photographic atlas of North Florida estuarine phytoplankton and a summarization of life history relationships and associations with various environmental conditions

[From the U.S. Government Printing Office, www.gpo.gov]

A PHOTOGRAPHIC ATLAS OF
NORTH FLORIDA ESTUARINE
PHYTOPLANKTON
AND A SUMMARIZATION OF LIFE HISTORY
RELATIONSHIPS AND ASSOCIATIONS WITH
VARIOUS ENVEPONMENTAL CONDITIONS

b y

Robert J. Livingston and A. K. S. K. Prasad

Center for Aquatic Research and Resource Management
Florida State University
Tallahassee, Florida 32306

December, 1989
QK
933
.L58
F6
1989

A PHOTOGRAPHIC ATLAS OF
NORTH FLORIDA ESTUARINE
PHYTOPLANKTON
AND A SUMMARIZATION OF I= HUSTORY
RELATIONSHIPS AND ASSOCIATIONS WITH
VARIOUS ENVIRONMENTAL CONDITIONS

b y

Robert J. Livingston and A. K. S. K. Prasad

Center for Aquatic Research and Resource Management
Florida State Tiniversity
Tallahassee, Florida 32306

December, 1989

PREFACE

This report is based on years of studies in the Choctawhatchee River and
Bay system and the offshore Gulf of Mexico. The data are currently undergoing
analysis, modelling, and publication in a series of reviewed scientific
publications. This data base is part of a more extensive research effort by the
Center for Aquatic Research and Resource Management.

ACKNOWLEDGEMENTS

The data for this project were the product of studies funded by the
Northwest Florida Water Management District, the Florida Department of
Environmental Regulation, and the Center for Aquatic Research and Resource
Management (Florida State University). Special thanks goes to Mr. J. William
McCartney, Mr. Walter Francis Spence, and the honorable James G. Ward who
contributed to the conceptualization and the continued funding of the project.
The staff people of the Northwest Florida Water Management District, with
special thanks to Mr. Doug Barr, Mr. Tom Pratt, and Mr. Augustin Maristany,
have been a source of invaluable support.

Funds for this project were provided by the Department of Environmental
Regulation, Office of Coastal Management using funds made available through
the National Oceanic and Atmospheric Administration under the Coastal Zone
Management Act of 1972, as amended. Mr. James W. Stoutamire administered
the grant on behalf of the FDER.

The research team of the Center for Aquatic Research and Resource
Management who have participated in this part of the project is as follows:

Administratiy-Q support

Glenn C. Woodsum
J. Michael Kuperberg
Delia L. Giblon
Lynne Figueroa

Scientists

Christopher C. Koenig (fish biology)
Gary L. Ray (macroinvertebrates)
William R. Karsteter (aquatic insects)
John Epler (aquatic insects)
Manny Pescador (aquatic insects)
.Frank Jordan (fishes)
Sean E. McGlynn (chemistry)
Tom Pratt (NWFWMD; hydrology)

Statistical/computational team

Loretta E. Wolfe
Jane M. Jimeian
Dorinda L. Dugan
Monica L. Britt
Joseph Bruce
Virginia E. Wotring
Heidi P. Cordero
Ralph A. Zuniga

Field sampling and laboratory data proce

William P. Greening, Jr.

Sample processing

Hampton E. Hendry
James A. Nienow
Carlianne Wilson
Brian K. Alexander
Kelly C. Bousman
Christy A. Chism
Elizabeth Dwyer
Vincent M. Gendusa
Robert S. Johnson
Lynne M. Kurtz
Jonathan G. Lammers
Jill M. Nast
Susan R. Pollack
Karen R. Quist
Mellissa Diane Rehder
Linda B. Sharer
Keith F. Zeitlin
Amy Leinbach
Alexander. Castiello

LIST OF FIGURES

Figure 1: Maps of the study area for the phytoplankton collections including the
Choctawhatchee River and Bay systems and associated Gulf areas
(Station-specific data listed in Appendices I and 11)

Figure 2: Summary data (12 month averages) of physical-chemical factors
taken in the Choctawhatchee Bay system from September, 1985 through
August, 1986.

Figure 3: Summary data (12 month averages) of chlorophyll a taken in the
Choctawhatchee Bay system from September, 1985 through
August, 1986.

Figure 4: Summary data (12 month averages) of particulate organic matter
taken in the Choctawhatchee Bay system from September, 1985 through
August, 1986.

Figure 5: Summary data (12 month averages) of phytoplankton numbers and
species richness taken during the day in the Choctawhatchee Bay
system from September, 1985 through August, 1986.

Figure 6: Summary data (12 month averages) of physical-chemical taken
in the Choctawhatchee Bay system from September, 1985 through
August, 1986.

Figure 7: Phytoplankton data (64grn nets) concerning numbers (X 1000) per
M3, species richness, and Shannon-Wiener diversity taken monthly from
September, 1985 through August, 1986.

Figure 8: Phytoplankton occurrence as a function of distributions of salinity,
dissolved oxygen, Secchi depths, orthophosphate, nitrate, ammonia, and
chlorophyll a. The numerically dominant phytoplankton species (16) are
tested as possible indicators of water quality phenomena in the
Choctawhatchee Bay system from September, 1985 through August,
1986.

LIST OF TABLES

Table 1: Systematic review of phytoplankton taken with 25 ltrn nets in the
Choctawhatchee River system.

Table 2: Cluster analysis (Czekanowski similarity coefficient; flexible grouping
strategy with beta = -0.25) of stations by sampling parameters
(Choctawhatchee estuary, all dates, surface and bottom station data
pooled).

Table 3: Metal accumulation index (A) computed for seven metals at 25
locations sampled in sediments of Choctawhatchee Bay in April, 1987.

Table 4: Systematic review of phytoplankton taken with 25 and 64 gm nets in
the Choctawhatchee estuary from September, 1985 through August,
1986.

EXECUTIVE SUMMARY

An-analysis was made concerning the phytoplankton taken in the
Choctawhatchee River and Bay system and offshore portions of the Gulf of
Mexico. A photographic atlas of the algae taken in the Choctawhatchee Bay
system was featured along with a determination of how well such organisms
were indicators of water quality in this estuary. Various community parameters
such as numbers per unit volume, species richness, and species diversity were
useful in identifying specific water quality conditions associated with cultural
eutrophication in the bay system. Some dominant species were identified with
specific water quality factors although the use of single species indicators of
such water quality is complicated by the fact that many estuarine species have
broad tolerances to such conditions. A combination of single species and
community factors may be useful as indicators of various forms of aquatic
habitats including water that is affected by anthropogenous acitvities. Data
analyses will continue with an emphasis on combinations of moderately
abundant and rare species as possible indicators of water quality from fresh
water to estuarine and marine systems.

TABLE OF CONTENTS

Page

Preface
Acknowledgements
List of figures iv
List of tables v
Executive summary vi

1. Introduction ....................................................................................................................1
A. Qualitative algal indicators
B. Choctawhatchee, basin characteristics
C. Geomorphology
D. Climate
E. Land use and wate-r quality

11. Methods and materials ................................................................................................. 12
A. Water quality
B. Phytoplankton

111. Photographic atlas ........................................................................................................ 18

IV. Analysis of species distribution .................................................................................. 19
A. River algae
B. Estuarine phytoplankton distribution
1. Water quality
2. Taxonomic review: species occurrence
3. Algae as water quality indicators

V. References ...................................................................................................................... 31

VI. Appendices .................................................................................................................... 35

vii

1. INTRODUCTION

The use of algae as indicators of water quality is well
developed in the scientific literature (Schubert, 1984) and has been
developed along both qualitative and quantitative lines. The
background of such methods in the field includes a general
acceptance that clean water supports speciose assemblages of algae
whereas polluted water tends to reduce the number of species and
increases the relative dominance due to the survival and well-being
of a few resistant forms. There is, however, relatively little
information -concerning the microalgae of the major drainages in
Florida, especially along the northern gulf coast.

A. Qualitalive algal indicators

Phytoplankton are microscopic aquatic plants that are usually
free-floating and suspended in a series of habitats, "having little or
no resistance to currents" (APHA/AWWA[WPCF, 1980). The use of
such organisms as indicators of water quality is well established. This
includes the use of various species that either flourish in highly
eutrophic conditions and/or are sensitive to various types of toxic
wastes. According to such information, there are certain algal
indicators that can be used in the evaluation of water quality. Clean
water indicators include Melosira islandica, Cyclotella ocellata, and
Dinobryon spp. Indicators of contaminated water include
Aphanizomenon flos-aquae, Microcystis aeruginosa, and Nitzschia
palea. Some forms, such as the former two species, can be associated
with algal blooms and anoxic/hypoxic conditions. According to
APHA/AWWA/WPCF, 1980, the following groups can be used as
indicators:

Clean water, algae

Agmenellum
Ankistrodesmus
Calothrix
Chromulina
Chrysococcus
Cladophora
Coccochloris
Cocconeis
Cyclotella
Entophysalis
Hildenbrandia
Lemanea
Meridion
Micrasterias
Microcoleus
Navicula
Pinnularia
Rhizoclonium
Rhodomonas
Staurastrum
Surirella
Ulothrix

Pollution indicators

Anabaena
Arthrospira
Carteria
Chlamydomonas
Chlorella
Chlorococcum
Chlorogonium
Euglena
Gomphonema
Lyngbya
Nitzschia
Oscillatoria
Phacus

Phormidium
Pyrobotrys
Spirogyra
Stigeoclonium
Tetraedron

There are problems with the use of such indicators. Because of
the temporal and spatial variabilityl the definition of water quality
by microalgal species can be difficult. In rivers, the origin and level
of exposure of algae to various water types remains problematical. In
@estuaries and marine systems, complex currents also can preclude
exact definitions based on the presence and/or absence of algal
indicators. Presence/absence data are qualitative; in this way, the
use of indicator species is limited by the problems associated with
qualitative methods of assessment. Such assessments cannot lead to
the evaluation of cause-and-effect relationships. In addition, process
oriented functions cannot be determined using indicator species.

On the other hand, the use of algae as indicators of water
quality has a well established basis (Stoermer, 1984). Qualitative
data can be used to determine the species associations of a given
aquatic system. The use of correct systematic data is crucial to the
determination of the ecosystem structure. Such information is
important in the interpretation of process -oriented data. For
instance, due to gas vacuole formation, an ability to escape nitrogen
limitation , and a colonial growth habit, blue-green algal species of the
genera Anabaena, Anacystis, and Aphanizomenon are considered
indicative of water pollution of various types. Some forms of blue-
green algae also emit toxins that can have an adverse effect on other
species. Thus, the blue-green algae are important in the evaluation of
water quality. In marine systems, dinoflagellates have been
implicated in the release of toxins. Flagellates can cause problems in
brackish water ponds. The species Oscillatoria rubescens is an
indicator of the eutrophication of oligotrophic lakes (Edmondson,
1972). There is a succession of algal species as eutrophication
proceeds. According to Reddy and Venkateswarlu (1986), pulp mill

effluents caused certain changes in riverine algal assemblages. There
were reduced numbers of phytoplankton in the effluent channel; The
Cyanophycean types were dominant in such areas with an almost
total lack of green algae. Oscillatoria spp were the dominant species
in the polluted areas with Rhopalodia gibberula and Nitzschia palea
as the primary diatom species. Premila and Rao (1977) showed that
blue-green algae (Oscillatoria nigroviridis) were indicative of waters
characterized by sewage relative to less polluted areas. Low salinity
in such areas tended to encourage this species along with the sewage
effluents. Blue-green algae are also abundant in marine areas under
natural conditions (Potts, 1980). Qualitative signs can- thus be used in
the identification of water quality problems.

Diatoms are useful in the analysis of the history of a given
water body (Stoermer, 1984). According to Schoeman and Haworth
(1984), diatoms can be very useful under certain circumstances in
the evaluation of water quality. Such algae are: easy to collect;
cosmopolitan; responsive to environmental conditions (short and
long-term); relatively well understood ecologically; suitable for
'historic surveys; suitable for diversity analyses. Disadvantages
include the fact that identification is highly technical and requires
considerable expertise. Patrick (1984) has reviewed the manner in
which shifts of diatom assemblages can be used to indicate changes
in ambient water quality conditions. Different species of diatoms
flourish under varying concentrations of nutrients and pollutants.
Often, the response of a given population may be indirect, due to the
effects of increased or decreased competition from species that are
affected by water quality conditions. Geissler and Jahn (1984) have
reviewed the infraspecific taxa with respect to morphological and
ecological differentiation. Sullivan (1984) showed that diatoms can
be quantitatively used in freshwater systems but that the use of
such populations in estuarine and marine systems is much less well
developed and understood. Salinity changes, together with highly
variable (spatial and temporal) distributions of diatoms, have not
been well studied. Thus, the actual relationships of diatoms to water
quality in estuarine and marine systems are not as well developed as

they are in freshwater areas. Wilderman (1 984) has outlined the
indicator diatoms for spatial and seasonal variation. Although there
are identifiable salinity and temperature preferences of estuarine
diatoms and that seasonal changes in such indicators are relatively
easy to establish, the distribution patterns within seasons are more
difficult to -interpret. Euryhaline species complicate the process in
that the are not useful indicators of salinity distribution. The
complexity of the diatom assemblages in estuarine areas was
illustrated by Squires and Sinnu (1982) who showed that various
factors are related to the determination of diatom distribution.
Currents and salinity were important factors in the -determination of
diatom assemblages in the area of study. Marshall (1982) showed
that the marine diatom distributions in the Gulf of Maine were
related to the location of large bay systems and the Georges Bank.

Maestrini et al. (1084) gave a complete review of the use of
algae as indicators of water quality in marine systems. The authors
point out the various problems of trying to make associations of
water quality factors (and nutrient processes) and descriptive algal
data. Differences in essential nutrients, the physiological state of the
indigenous algal populations, and other factors that are difficult to
measure all contribute to the complexity of causal relationships in
estuarine and marine systems. The authors advocated the
experimental (e.g., bioassay) approach to evaluating water quality
relationships with phytoplankton. Actually, both methods
(descriptive and experimental) are necessary for a real
understanding of how aquatic systems function. In any case, an
evaluation of the species composition of the algae in a given system
represents an important first step in the evaluation of existing water
quality.

The toxic effects of contaminants on algal communities in the
field have been addressed only recently. This entire subject is, in
fact, relatively complex and poorly understood. At the ecosystem
level, the natural interactions (physical and biological) of the
phytoplankton in freshwater and marine systems along the northern

Gulf coast of Florida remain virtually unknown. Unless ambient field
conditions are established, the influence of human activities on algal
associations in a range of habitats will be difficult'to evaluate. This
atlas is an attempt to establish the ambient conditions of
phytoplankton assemblages in a series of aquatic habitats
(freshwater, estuarine, marine) in a relatively unpolluted (the
Choctawhatchee River-bay) system with some attention to the
associated offshore (Gulf) region.

B. Choctawhatchee Basin characteristics

Detailed reviews of the basic geomorphology and hydrology of the
Choctawhatchee River basin are available (Abbot, Merkt & Company, 1960; U.
S. Study Commission, Southeast River Basins, 1963; Federal Power

Commission, 1966; Soil Conservation Service, U. S. Department of Agriculture,

1975; Northwest Florida Water Management District, 1980, 1988; U_ S. Army

Corps of Engineers, 1980).

The Choctawhatchee River system represents the main source of fresh
water for the Choctawhatchee Bay system, and is the fourth largest river in

terms of flow volume in the state of Florida. The Choctawhatchee River is

formed by a series of tributaries in Alabama and Florida (Figure 1). The

headwaters are in Barbour County, Alabama. The major tributary, the Pea

River, joins Whitewater Creek to form the western wing of the Choctawhatchee
drainage basin as it joins the main river just south of Geneva, Alabama. In

Alabama, the Choctawhatchee River runs for about 88 miles draining

approximately 2,500 square miles. In Florida, the river then runs another 87

miles to drain about 1,500 square miles. Here, the major tributary is Holmes

Creek. Other major tributaries to the Florida portion of the river include Wright's

A L A B A M A

Wrights Creek

T
Choctawhatchee River

69
N

Bonifay
6
68
V.,@I IF
Caryville
rr
I )V

I- Ff
)e Funiak S rings

64
63 Holmes Creek

C;
.1t
k
Choctawhatchee River
61
A
Ebro.
,'hoctawhatchee Bay
... tl

a
, @ A
60

-4-ILL".
Map showing placement of sampling stations in the
T. Choctawhatchee River system.

Map showing the various Sub-basins within the lower
Choctawhatchee River system (courtesy of the Northwest Florida
Water Management District, Mr. Tom Pratt).

CHOCTAWHATCHEE.
RIVER TRACT

0 10

Cal Miles

z
LO
WALTON 8' HOLMES

WESTVILLE
CARYVILLE
z 0
V
DE FUNIAK PONCE
SPRINGS DE LEO 7

AR YLE
L

8
z
C1

WASHINGTON

HOLMES CRL-EX
WALTON
z

28
81
3

FREEPORT

20 BRUCE

..........

CHOCTA HATCHEE
DAY
BAY
98

to
cli

OP
4/co WEST SAY

R19W R18W R17 Rlew,/
Map showing extent of the recently purchased wetlands (state
purchase of the Choctawhatchee River Tract; Northwest Florida
water Management District) within the area of study.(courtesy of
the Northwest Florida Water Management District)

EGLIN AIR FORCE BASE

NICEVILLE

VALPARAISO'

A
------------------------
AWHATCHEE -------
VAOCT- ArENWAV
C,

FT.,WALTON
BEACH @A A
0
A
A
DESTIN

GULF 0
ICO
0 Biological and Water Quality Sampling Station
A Biological and Water Quality Sampling Station for
Sediment Chemistry

Location of Sampling Stations

Computerized map of habitat distribution by
station in the Choctawhatchee Bay system.
CHOCTAWHATCHEE BAY
Habifaf Disfribuflon

By STATION

28
29A 27 13
0 14
18

40 33 21
4A 15
31 19
41 37 34 25 22 12
M
42 38 32 6
36W&E 20
43 39 35 26B 23
4

DEEP SHEV/SLOPE,V
SHELF/SLOPE,UN-V BAYOU
OTHER

Place nameslapproximate stationlocations; S - sed
Choctawhatchee Bay Project 19815-1986 W = wate
sed
sed
3 3

Basin Bayou
Kilometers Freeport

0
14 Alaqua Point
Ijamock poliNt La Grange! %,6YOU

Crassy Cove

O-S, P
0-5 D, P
cboctawhatthpe Day 15 6

12 jol I
io 0
tkf 2

O-S
17 3

Sante Rosa Beach

Sandesti(I
Point Was

U.S. 331

ximate station locations:
Place names/appro
Choctawhatchee Bay Project 1985-10,86 W
D

Valparaiso Rocky Bayou
29A 27
Toms Bayou Niceville
S, w

S
weekley Bayou 28
N 30 S
Garnier Bayou
Buccaroo Point S, D,P
31
Eglin Village Stake
Oe

24 C)
ocean 40 Shalimar 33 ChoctawhatChee Bay 24A
t

A
Of S, P
41 25
S
37 P
CO 7%
34 32 1@
S P S 26AO 22
For walton Beach 38 26B 26 LD Piney point
0
If S
S 39 35 Destin k 1,701toq 10
Santa ROS 42 "01?o 407 11.
0 Old Pass Lagoon 'bat'It
Santa Rosa Island
43

36W 36

23 In the U.S. Coast Guard Light List.
POLLUTION REPOFITS
Report all spills of oil and hazardous substances to the 2 1
22

L National Response Center via 800-4244802 (loll free), or 20,,'
to the nearest U.S. Coast Guard facility If telephone com- I
municallon Is Impossible (33 CFR 1153).

")UMPING
N
:signated for 14
ig. Such use 5
,tion of such
uthority for
10
9__

7
a contained In 40
n concerning the
5-
'the siles may be 0
'n Agency (EPA). 4- 0
3-
,as of EPA offices.

LORAN LINEAR INTERPOLATOR

10 Pot A0 L10 AEA0 R an
379:"-..

00 16,
f NOTE@E.
T-A Ck
t... ;tA Port St. Joe Is In the
15 'r it
'2 Eastern Standard Time Zone.

Spr@irf W.,H.' Cr..
36 E Ire 16M
'14:
It pn SLj.. Op F1 11M 0-1
28-- \ - -*,r 111!
Xul,xp d'#PM !V9, PA 9
V. 7
'0
to
@113 -
t?CxFx 0 P
Al
4 22 x"1111 it FIN
I
14 "OR
Ei- W \ III HORN
Iles no
@R
kl@ Mill 9 -V'
S 134-
DA

ch
12%
6;@ PA, 4
00
04 JXI , X
I, k 114 4.1
jr 14
J3
N 14
Q
16 th
0
4
(sad &e A
A) 08 R Bn
FA

-0

22 10
7,
13 PA
12'
137 t
I % 17, 14
'o

32
it
PA PAA
282,-
@7X!8

04 2
00 YS_
272
iu'9 Ire
@?O' /r4. U 17V 13
1112
3 9
<
15
476 '\
4 2
1710 @Z rjos/vc
6
1 64 6
@WING 33 16
4
ANCAC r1l @4 00
29
Ur
I DISU011F
Z q-50
k.000

16 3
0 14 rs cjunl-n IiNo@e),
e a 0
%3A lilt I ilIl 17% 71@ I
'0
%\ L.? r"@ i \ I I, '< 'i '\ .
30
16/v@
I \ I / . Brad
V
_42
NN" 170
< 32\
t A 5 INI A
2 it

5 LJ 0- #E@
G LORAN LINEAR INTERPOLATOR
f-
Atjr. "jo cA,,,;. Stlfarlm
1142

R
2 tent 1,6,5).
Occ 4se/c 92
Fl
ey.4I 2.
21
Ivy
2. 21 U
PA
NOTE C 11 3.
Port St. Joe is in, the If
FI
.astern Standard Time CA'
one. 2, 1,
Jeg

S
Nfu,
J@ 24 2" 2 R-24*1 4,1
21 31 21
4,- a 4,
C
3 n 21"A
21 4
38
tr ` @:
Loki WVAiC0 GP A M 158W 115ft 14M IL 53,
V %@
0 3-
L A 0,
3, 4,-
21 5: 64BELL 6: u
01 0 2 4, 41 4; 6
R 7 5. S 6:
Ff Set: .6. 6., Leg 1, day 1
Bi LL 53
3,
44 PA
21 6 61, 7,
Sr Vzwr,,,,. 73
6; 8;
:t3l.
2
Us. chwf 3j 61 R PA
0 TR
@,*'A 4@_a% I . Ok FI U looff 5M 'K'
0 71 H
0;i@
'. IVA op 9 (Air Force 6, 7
,Vz@ DANGER Ar. 204,7,2 4- 73
a rlA 9
r
art
%%Mrr@ If-C ro: 31 art
41 63 0.5 9 1'
04
PA
-,,' -PA
4' 31 2, 84EL L A-V 8, 9
& 6 9
& 'i@ge 0 10
pe St qva
-4
w Or -M-
7 (s- I IC4 10
Is 1011.014ORN 101
@r@z 1 10 -,(Air Force r 1 350 S' Ce
5k Leg 2, day 1 IV Ok F) Lt I 07ttS 0.
9
'4@ @/. Y M @'@ 1, 11 t I I 1(0)
'Caotj
1,01, '.l' ..L -I - d)l ,/C.1
4 00%zr PA 7: -10 2
0.
21 r 51 f 2'
9 13 -?o
0, 7
Gr 13 - 12
12 0 13 2 12
.7 51 7 'z 13
31 .0 W, kv
13
x 30
11 13
0%, 3
104 ETiC "")3
11 12 4-
14
12 3
7,
Ho 14
2
RM 100f., M Air Force moi.
lk 12 \I' H 4 101It Fl Lt 100ft % 2
13
rz 14 (A r
"@l R 6*oc SEU 15 S
15
0

mbers shown with Fish Haven in the Safety Fairway area
is 47 feet.
SATION CY11PE ST. GEORGE I
ard Light List for
i concerning aids AERA + NOTE S
ROL W&C
Aron, -,.td Regulations for Ocean Dumping Sites are M
__D @R_, contained in 40 CFR, Parts 220-229. Additional Seal
RrS TRIC, information concerning the regulations and
?f-A 204.134 see "fe XY tchii 11385) fewrements for use of the sites may be ob- North
R TR CArO C 21,Lj*1zr.,%.T CJ1E 2 tained from Environmental Protection Agency
A) (WD S)
1260 kHz0 kh-,r 11385) (EPA). See U.S. Coast Pilots appendix tor so UNIII
addresses of EPA otlices.
NK
............ T NK ATMEX
,it 44
a-TB
A, (For
A_ .... �z 615 TR
-q01 if Roating
-sw buoys
101 1011 13\ 10i 8 See L-80,
if tirs Sh -4 jo scale harbo
14 12 titI _J2 S12 _@Lol 101
maintained
\12 13
12 P 101 7.
-,0 - - - - - - 7.-"j ? \14
12 k4' 12 12 -71 1@
Leg 2, day 4 t;t 9
12 T
7@ I @, -
12
S \ @14
.,10 12 1 14 Leg 2, day 3
12'- 2 1
A 16 f? 16 2 7
Wks 13 . .14 15 reported PROHIBITM AR
1*4 16 \1 4 204.126
13 16 15 1.4 1 14 '13 12:_ 1 J?D 10
Is \ 7 See
5 16 1 1 ?8WA
15\ 14 1.15 12 - 11.6 ?ARK
is C sub C.6 16 17 17 Is Sh
13
6 14 12
16 17 X Is'.
la 13
17 is 10
18 17 16 0, o..
Sh
19 6 Sri 16 14
26 21 7 22 v..t Is 13
23 3 2'--
PA 5 1
21 'A
27 29. 21 U
% - A 4
24 18 Is 15 IS ==@b@A@ \'?DV"p S"rr
24 9 1\ @ 14J."'A l2wo@tj-@
26 19
35 16 11389',. -@r
24, 22 21 3 &Pi 16 6 14 0'
-,_38\ 24 26 19 PA .:@,,1,101
Ch.7rt 11288 17
41 25 1-16 i
28 27 AA
22
27
2X CAU 16
34 R 23 17
-2-9 MISSIL A 21
=--2 7 24 _15
;)04 5 . .....Agy
f4
0- - =
_f, 2 1 P AR
Isee 204126 4
62 56 !46, 45 17
3t, 12
28 24 17 nole_A,4@"
-4-2- 19 12m, 14
53 Is Is 17
4, --21 21 \ \ - S, ._ 171
P 43 16
4\0
PD 25 19 is 16
21- 16
IC.
65 5 35

16
Leg 2, day 2 '9
41 q9 38'.. 17
58
.?0 41% 1 29 22 14 16
37
51 Is
9
56
/1", 0 N i \-.--24
`48' 44,
4 23-- 22
, i... 21
0 _Az - < r
28 17. C5
84 63 ab C.
_-57 \47 23 19
77
21
Jo 36 23 - I
0 Is
- 17 Is, -
56 27
Art fRep 1956) PA-2C',
71 44 27@
PA 22 22
17
:29 0
21

Creek, Sandy Creek, Bruce Creek, Seven Run Creek, and Pine Log Creek.

Sampling stations were placed on each of..these tributaries in addition to main
stem (Figure 2). Such tributaries represent a major part of the basin for the
Florida portion of the river (Figure 3). These stations also include major
sections of the wetlands recently purchased by the state of Florida (through
negotiations by the Florida Northwest Water Management District) as shown in

Figure 4. The average flow rate of the river ranges between 5,500 and 7,000

cfs (U.S.G.S., 1978) with low flows approximating 3,400 cfs and high flows of

26,000 cfs (Ross et al., 1974).

The Choctawhatchee Bay system (reviewed by Livingston, 1986a) is an
east-west oriented estuary with the primary freshwater input at the east end via
the Choctawhatchee River (Figure 1). Fresh water also enters the system along

a series of smaller drainage areas primarily in northern sections of the bay.

River flow peaks occur during winter-spring months with low flows in the
summer and fall. There is a shallow shelf that is located around the fringes of
the bay; sandy sediments occur here. The central portions of the bay are deeper
and are characterized by fine-grained, highly organic sediments. The spring

temperature transition occurs in March with peaks of temperature from June to
August. The fall transition occurs in November with winter lows from December

to February. Salinity gradients follow trends in river flow with the lowest

salinities found from December through April. Pronounced vertical salinity

stratification occurs in large portions of the bay (particularly in western and

central areas); during warm periods, such statification is associated with
hypoxic conditions at depth. In August, 1986, virtually the entire bay was

hypoxic to anoxic at depth. Such hypoxia occurs in various western bayous and
lagoons (lower Rocky, Boggy, Tom's, Garnier, Cinco, Old Pass Lagoon). Such

areas are adversely affected by storm water runoff and other factors such as

marinas (Old Pass Lagoon). Nitrogen levels are highest in western sections of

the bay and phosphorous is highest in Old. Pass Lagoon, Lower Rocky Bayou,

and Boggy Bayou.

Q. Geomorphology

Surface sediments, composed of lime accumulations and/or sedimentary

deposits of sand, silt, or clay, rest on a base of crystalline rock some 2.500 to

4,000 feet below (U. S. Study Commission, 1963). The lower coastal plain is

flat and sandy with beach ridges extending to elevations of up to 200 feet. The

Tertiary limestones, forming the principal artesian aouifer in this part of Florida,

form outcrops at or close to the surface of the bed of the Choctawhatchee River.

The Ocala limestone, with its sinkhole topography due to the solution of the

limestone bedrock, forms a major portion of the Deadening Lakes region of the
Choctawhatchee drainage in Washington County, Florida at the southern end of

the river.

D. Climate

The Choctawhatchee, River basin lies in a south temperature region

characterized by mild winters and hot/humid summers. Some moderation of

these climatological characteristics occur in the coastal region of the basin. The

average temperature is 68 OF with a range of 50 OF in December to 81 OF during

July/August (U. S. Study Commission, 1963). Average annual rainfall varies

from 52 inches in the upper basin to 62 inches in the southwest portion of the
system. Maximum average annual precipitation approximates 85 inches (1929)
with the minimum such levels about 26 inches (1954). The wettest months are

June-September. The Floridan Aquifer provides the major source of water to

the river system which includes numerous streams, lakes, and springs. The

maximum 24-hour precipitation was recorded as 20 inches at Elba, Alabama in
March, 1929\,(.U. S. Study Commission, 1963). During the spring of 1975, there
was heavy rainfall and flooding (17.7 inches in a 24 hour period in April, 1975);

this stimulated the evaluation of storm control measures (U. S. Department of

Agriculture, 1975) due to what were perceived as major flood and erosion

damage. Various flood control measures have been proposed by the U. S.

Army Corps of Engineers for the Choctawhatchee basin (Northwest Florida
Water Management District, 1980). Such proposals include structural and non-

structural m ethods along with land use regulations.

E. Land use and water quai Ut

Land use within the Alabama portion of the Choctawhatchee basin is

dominated@,by forestry (51.7%) and agriculture (cropland, 30.6%; pasture,
11.6%) (Alabama Water Improvement Commission, 1976). There is relatively
little urban development in the region (3.2%). In Florida, the basin remains
largely u ndeveloped with forestry (58.4%) and agriculture (25.7%) as the major
land uses (-F\Iorida Department of Environmental Regulation, 1980). The largest

cities in the Choctawhatchee basin include Chipley, Bonifay, and Defuniak

Springs. The western section of the bay is becoming highly urbanized with
stormwater runoff bringing nutrients and various pollutants into the system.
Such urbanization is still no present in eastern sections of the bay so an east-
west gradient of water quality exists.in addition to the above-noted salinity

gradient.

The major sources of pollution are agricultural runoff, sewage

discharges, and minor industrial effluents in the river basin and stormwater

runoff and marina wastes in the bay system. According to the Florida
Department of Environmental Regulation (1980), the mean dissolved oxygen

levels in the river were above the state water quality criterion (5.0 mg/L). The

pH levels in the river varied from 6.3-7.6. There were 'low' levels of Kjeldahl

nitrogen (mean X = 0.03-0.05 mg/L), nitrate/nitrite (mean X = 0.06-.26 mg/L),

and total phosphorous (mean X = 0.03-0.05 mg/L) throughout the river with a

decreasing trend toward the mouth of the river. Concentrations of mercury,

cadmium, and lead were in excess of the state water quality criteria. High levels

of fecal coliform bacteria were noted near the town of Ebro due to what is
thought to be agriculturai 'runoff (Florida Department of Environmental

Regulation, 1980). Trend analyses indicated increasing total phosphorous,
decreasing nitrate-nitrite, increasing average dissolved oxygen, and decreasing

mean pH. Available data indicated "generally good water quality in the

Choctawhatchee River south of the Florida-Alabama State line" (Florida

Department of Environmental Regulation, 1980).

More recent studies show significant water quality degradation in the
lower Choctawhatchee basin. According to a recent update of this report
(Florida Department of Environmental Regulation, 1986), the Choctawhatchee

River basin now exhibits more water quality problem areas than other areas of
low population density. There are high ambient values of nutrients in Wright's
Creek near Noma, Florida due to agricultural runoff and possibly the numerous
impoundments of this area. Upper Holmes Creek has water quality problems
due to discharges from Graceville (Little Creek), Chipley (Alligator Creek),
Vernon (Little Branch), and Bonifay (Camp Branch). Such problems are due

largely to sewage discharges. Holmes Creek also receives runoff from

agricultural areas such as hog farms. West Sandy Creek also has degraded

water quality due to sewage from Defuniak Springs and Bruce Creek receives

effluent from a chicken processing plant. There were violations of standards

concerning dissolved oxygen, NH3, coliform bacteria, and BOD5. Bioassays

indicated toxic wastes. One area of Bruce Creek, near a 331 truck stop, has

been polluted with oils and diesel fuel. The lower Choctawhatchee River was

considered having "significant" biological degradation with a low number of

macroinvertebrate species (Florida Department of Environmental Regulation,

1986).

11. METHODS AND MATERIALS

The general distribution of sampling sites is given in Figure 1. The field

sampling program included different variables that were to be evaluated

together to determine specific ecological features of the Choctawhatchee

Drainage system. In the river, such variables included habitat characteristics,

flow rates, water quality and sediment characteristics, mass flows of nutrients

through the system, and biological features (e.g., phytoplankton, infaunal

macroi nve rte b rates, epifaunal macroinvertebrates, fishes, food web

organization). A sub-topic for analysis included the relationship between the

various tributaries and the main stem of the river. The relationship of specific

state variables such as river flow and wetlands distribution with the various

biological features of the system were of major concern in this study. The

sampling protocols for the estuary and offshore (Gulf) areas followed along

similar lines (Appendix 1).

A. Water quality

The methods used in the water quality analyses are detailed in Appendix

11. Some additional nutrients (especially phosphorous compounds) were added

to the original protocol.

River stations were sampled along with a series of established bay
stations to evaluate the influence of the river on the bay. Routine water quality
measurements included surface and bottom temperature, conductivity,
dissolved oxygen, depth, and Secchi readings. In addition, three 2-1 samples of

water were taken from the surface and bottom; these samples were iced and
immediately shipped back to our Tallahassee laboratory for the analysis

described in detail in our protocols.

B. Phytoplankton

Phytoplankton samples were taken with 15.2 cm (D) plankton nets (28gm
mesh in the river and 64gm nets in the bay. In the river, the nets were
suspended close to the surface on a line weighted at the bottom and attached to
a float at the top. Three nets were set across the main stream for one hour. The

center net had a flow meter suspended just below the net to quantify the volume

of water sampled. At the end of the sampling hour, the nets were rinsed into

numbered jars and preserved in 5% formalin (nets were numbered _ 1-3, which

corresponds to left-right across the stream). In the bay, samples were taken

with nets and with pumping as described in Appendix A. The eastern stations

(3, 7,15) were sampled for two years with both 28 ILm and 64 gm nets. The

remaining phytoplankton stations (Appendix 1) were sampled with 64 lam nets.

The volume of each sample was measured in a graduated cylinder. The

sample was then stirred with a magnetic stirrer for 1-2 minutes, and a 0.1 ml

sub-sample was pipetted out. To limit clumping and cell damage, the stirrer

was turned off between sub-samplings. Each sub-sample was placed in a
Palmer-Mahoney counting chamber and the numbers -of cells were counted by
the 'strip' count method. In strip-counting, the top and bottom of the grid were

the 'count' and 'no-count' boundaries, respectively, and plankters were counted

as they moved across the center vertical line. Dead cells or diatoms with
broken frustules were not counted. Empty centric and pennate diatoms were

counted separately as 'dead centric diatoms, or'dead pennate diatoms' for use

in converting the diatom species proportional count to 'a count per ml. A

preliminary analysis (10 samples) was carried out to determine how many sub-

samples were necessary for each count. Three subsamples provided a number

within 22% of the mean of the 10 net sub-samples and this number was used

for all counts.

All samples were processed to species. Diatoms were cleaned using

heat if found by themselves. Otherwise, the sample containing various kinds of

algae were placed in a 100 ml beaker and most of the water was decanted. A

small amount of nitric acid was added and this solution was boiled for about 20-

30 minutes. The sample was constantly stirred until oxidation of organic matter

was complete. At this time, a small amount of potassium dichromate was added

until the solution was brown in color. The solution was then cooled and

decanted arid distilled water was added. This procedure was repeated until the

pH was 7. Alcohol was then added after the final washing and most of the water

was decanted. Diatoms were mounted with Naphrax. A 0.01 ml aliquot of
alcohol containing the cleaned diatoms was dropped on a coverglass so that
the diatoms spread evenly; after the alcohol evaporated, the coverglass was

heated so that the diatoms were incinerated onto the coverglass. The diatoms

were then mounted in the Naphrax. After preparation, electron micrographs
were taken on a Polaroid 4x5 Land film type 55/positive-negative using JEOL-
JEM-100CX11 scanning and transmission electron microscope operating at an

accelerating voltage of 20 KV. Light microscopy was also used with a Nikon

biological microscope fitted with a phase condenser; photographs were taken
on Kodak .35mm Panatomic-x fine grain black and white film using a Nikon

camera. Phase contrast illumination was used for diatom studies. Soft-bodied

algae were photographed using wet mounts in distilled water. Methylene Blue

and India ink were used to determine the extent of sheath formation. The

structure of the pyrenoid and enclosed starch caps, flagellar number and

insertion weire studied with 12 in KI solution.

Samples were brought into a field lab and studied in the living state with
a wet mount for determination of the general composition of the community.

Samples containing more than one group were split into sub-samples because
different methods were used for processing and identification. Such samples

were preserved in Lugol's Iodine solution. Various methods were used to

analyze the various phytoplankton components.

Identification was made from well-known manuals such as Germain

(1981), Patrick and Reimer (1966, 1974), Huberpestolozzi (1930-75), Hustedt
(1930), Prescott (1951), Smith (1950), Geitter (1932), Desikachary ((1959),

West and Fritsch (11927), Komarek and Fott (1983), Wolle (1894), Boyer (1927),
Printz (1962),' Ettl (11976), Iyengar and Desikachary (1980), Flint (1949), and
Philipose (1967). A complete review of the microalgae taken from the

Choctawhatchee River system is given by Prasad and Livingston (1987; An

Atlas of diatoms and other algal forms from selected drainage areas in central

and north Florida; unpublished report for the Florida Department of

Environmental Regulation).

A conversion was made of all phytoplankton data (numbers per species

/division). This was carried out using seasonal collections of phytoplankton

from various portions of the study area. R egressions were determined from the

experimental work (comparisons of the numbers vs. the ash-free dry weight

biomass). The following is the protocol used and the results of the regression

analysis:

PHYTOPLj%NKTON-WEIGHT REGRESSION PROTOCOL

1) Find Phytoplankton samples ( Rm 126 All should be labelled for
station, dale, net number, and net size ( 25 lurn

2) Weigh Glass-Fiber filters individually in standard weighing tins. Weigh
all filters and pans at least separated three times. Make sure to keep
accurate rocords and individually mark each tin. Include at least five filters
and pans to be used as controls ( untreated

3) Pour, sample through filter and wash any adhering material from sides
of sample via[ into filter with distilled water.. Pour distilled water alone
through five control filters. Make sure to put filters into pans they were
originally weighed in.

4) Examine filters and remove any detritus or zooplankters present

5) Plac-9 filters and pans in drying oven at 950C-1 OOOC for twentyfour (24)
hours. Remove from oven and let cool in Dessicator.

6) Weigh pan/filters on Mettler Balance to lowest possible weight.
Be sure all pans are cool before weighing since warm pans will adsorb
water from the air and cause the weights to fluctuate. Repeat weights on all
pans at least three separate times.

7) Place filter/pans in ashing furnace at 5000C. Burn to ash. Remove
filter/pans from oven and let cool in dessicator. Weigh as before.

8) Make sure to keep exact records and follow protocol.

0 % 0
M 0 0
W 2- 0
P-0
u Or EP
ap 0
Elm
m

0
0.02 0.04 0.06 6.08 0.10
Ashfree Dry Weight

All data were converted according to this regression.
0 %
13

r
M zp
@13

111. PHOTOGRAPHIC ATLAS

The photographic representations of various estuarine algal species are

presented in Appendix 111.

IV. ANALYSIS- OF SPECIES DISTRIBUTION

A. River alaae

Although this atlas will concentrate on the estuarine phytoplankton as

water quality indicators, a brief description of the river algae is appropriate. A

more detailed treatment of the subject is given by Livingston et al. (1988).

A review of the taxonomic organization of the river microalgal

components is given in Table 1. In terms of numbers of species and numbers of

occurrences in the data base, the Division Bacillariophyta (diatoms) is the most

dominant group. In part, this is due to the methods of collection and

preservation; such methods favor the collection and analysis of organisms with

hardened cell walls such as diatoms. Among the green algae (Division
Chlorophyta), the genus Scenedesmus is predominant followed by Closterium

spp. Among the blue-green algae (Cyanophyta), the genus Merismopedia is

dominant. The genus Dinobiyon was dominant among the golden-brown

algae (Chr)rsophyta). The euglenoids (Euglenophyta) and cryptomonads

(Cryptophyt,a) were not well represented in these collections. A review of the

algae found in the Choctawhatchee region has been given by Prasad and

Livingston (1987).

The numbers of microalgae in the main channel stations (70, 68, and 61)
were low relative to most of the river tributaries and bay stations. Such low

numerical -rlibundance could be a product of the higher flow rates at these
stations. Phytoplankton numerical abundance was particularly high in Pine Log
Creek, Holmes Creek, Wright's Creek, and the estuarine stations (3, 7, 15).

Table 1: .13ystematic review of phytoplankton taken with 25 gm nets
in the Choctawhatchee River system.

Systentatic review

Choctawhatchee River, day, surface, 25g san-ples

No. of occurrences
Division ... Cyanophyta
Class ...... Cyancphyceae (blue-green algae or cyanobacteria)
Order ...... Chroococcales
'Family ..... Chroococcaceae
Chroococcus sp. 2
Merismopedia glauco 4
Merismopedia punctata 1
Merismopedia tenuissima 4
Order ...... Nostocales
Family ..... Nostocaceae
Anabaena catenula 1
Anabaena sp. 3
Family ..... Oscillatoriaceae
Arthrospira sp. 1
Oscillatoria amoena 1
Pseudanabaena sp. 1
Division ... Euglenophyta
Class ...... Euglenophyceae
Order ...... Euglenales
Phacus sp. r258 2
Phacus sp. 1
Division ... Cryptophyta
Class ...... Cryptophyceae
Cryptomonas erosa 1
Division ... Dinophyta
Class ...... Dinophyceae (dinoflagellates)
Order ...... Gymnodiniales
Family ..... Gymnodiniaceae
Gymnodinium sp. 1
Order ...... Peridiniales
Family ..... Peridiniaceae
Peridinium sp. 2 1
Peridfnium sp. 2
Division ... Chrysophyta
Class ...... Chrysophyceae (golden-brown algae)
Order ...... Chrysomonadales
Family ..... Ochromonadaceae
Dinobryon'sertularia 5
Dinobryon sp. 1 1
Division ... Xanthophyta
Class ...... Xanthophyceae (yellow-green algae)
Order ...... Tribonemales
Family ..... Tribonemataceae
Bumilleria exilis 1
Division...Bacillariophyta (diatoms)
Class ...... Bacillariophyceae
Order ...... Pennales
Suborder ... Araphidineae
Family ..... Diatomaceae
Asterionella formosa 13

Ctenophora pulchella 1
Fragilaria brevistriata 21
Fragilaria capucina 7
Fragilaria constricta 1
Fragilaria construens 9
Fragilaria leptostauron v. dubia 1
Fragilaria elliptica 2
Fragilaria leptostaur6n 3
Fragilaria pinnata 27
Fragilaria construens v. venata 7
Fragilaria construens v. venter 13
Meridion circulare 4
Opephora americana 2
Opephora gemmata 1
Opephora martyi 16
Opephora pacifica 1
Opephora pinnata 3
Opephora schwartzii 6
Pleurosira laevis 2
Rhabdonema adriaticum 3
Synedra sp. 265 2
Synedra acus 20
Synedra ulna v. amphirh_yncus 5
Synedra delicatissima 9
Synedra filiforms 3
Synedra incisa 1
Synedra-ulna v. oxyrhynchus 19
Synedra rumpens 2
Synedra sp. 1 1
Synedra sp. 1
Synedra tabulata 3
Synedra ulna 75
Tabellaria binalis 1
Tabellaria fenestrata 26
Tabellaria floculosa 15
Tabellaria quadrisepta 19
Tabularia investiens 7
Suborder-Raphidineae
Family ..... Eunotiaceae
Actinella punctata 3
Eunotia alpina 28
Eunotia monodon v. major f. bidens 3
Eunotia bigibba 1
Eunotia diodon 4
Eunotia exigua 1
Eunotia faba 2
Eunotia flexuosa 6
Eunotia formica 22
Eunotia lunaris 12
Eunotia monodon v. ma' 1
-70r
Eunotia monodon 15
Eunotia naegeli 3
Eunotia pectinalis 89
Eunotia polydentula 1
Eunotia praerupta 7
Eunotia praerupta v. bidens 1
Eunotia pectinalis v. undulata 20
Eunotia purpu@�silla 1
Eunotia quaternaris 1
Eunotia serra 6

Eunotia sp. 2 1
Eunotia sp. 3 1
Eunotia sudetica 1
Eunotia tautoniensis 5
Eunotia pectinalis v. ventricosa 1
Eunotia zygodon 1
Semiorbis hemicyclus 1
Family ..... Achnanthaceae
Achnanthes affinis 4
Achnanthes lanceolata v. apiculata 81
Achnanthes austriaca 3
Achnanthes bottanica 1
Achnanthes clevei 33
Achnanthes conspicua 3
Achnanthes delicatula 7
Achnanthes lanceolata v. dubia 65
Achnanthes lancealata v. elliptica 8
Achnanthes exigua 39
Achnanthes flexella 20
Achnanthes peragalli v. fossilis 1
Achnanthes haukiana 2
Achnanthes lanceolata v. haynaldii 1
Achnanthes exigua v. heterovalva 2
Achnanthes hustedtii 9
Achnanthes inflata 1
Achnanthes lanceolata v. lanceolatoides 10
Achnanthes lanceolata 12
Achnanthes linearis 1
Achnanthes lanceolata v. omissa 17
Achnanthes peragalli v. parvula 2
Achnanthes peragallii 19
Achnanthes lanceolata v. rostrata 1
Achnanthes saxonica 1
Achnanthes sp. 1 1
Cocconeis dimunuta 15
Cocconeis disculus 5
Cocconeis pediculus 1
Cocconeis placentula 70
Family ..... Naviculaceae
Amphipleura pellucida 1
Amphora disculus 1
Amphora ovalis 11
Amphora pediculus 3
Anomoeneis brachysira 7
Anomoeneis serians 5
Anomoeneis serians v. brachysira 1
Anomoeneis vitrea 1
Brachysira apomina 1
Caloneis molaris 1
Capartogramma crucicula 49
Cymbella affinis 7
Cymbella amphicephala 2
Cymbella aspera 11
Cymbella cesatii 1
Cymbella cistula 7
Cymbella cuspidata 4
Cymbella delicatula 1
Cymbella gracilis 20
Cymbella helvatica 3
Cymbella hustedii 1

Cymbella lapponica 1
Cymbella leptoceros 1
Cymbella lunata v. lunata 1
Cymbella minuta 4
Cymbella naviculiformis 5
Cymbella sp.1 1
Cymbella subcuspidata 35
Cymbella tumida 13
Cymbella turgidula 1
Cymbella ventricosa 1
Diploneis elliptica 5
Diploneis sp. 1
Diploneis oblongella 1
Diploneis ovalis 3
Diploneis pazma 3
Frustulia rhomboides v. crassinerva 1
Frustulia rhomboides 83
Frustulia rhomboides v. saxonica 1
Frustulia vulgaris 5
Gomphonema acuminatum 3
Gomphonema angustatum 35
Gomphonema augur 1
Gomphonema gracile 12
Gomphonema grovei 4
Gomphonema intricatum 1
Gomphonema grovei v. lingulatum 7
Gomphonema minima 1
Gomphonema parvulum 3
Gomphonema truncatum 2
Gyrosigma acuminatum 27

Gyrosigma attenuatum 5
Gyrosigma kuetzingii 1
Gyrosigma scalproides 2

Gyrosigma spenceri 16
Navicula sp. 248 1
Navicula sp. 251 1
Navicula cf. ammophila 1
Navicula anglica 4
Navicula bacillaris 1
Navicula bacillum 1
Navicula begerii 1
Navicula capitata 26
Navicula clementis 8
Navicula clementoides 1
Navicula contenta 1
Navicula cohnii 1
Navicula constans 12
Navicula capitata v. capitata 2
Navicula cryptocephala 66
Navicula cuspidata 7
Navicula cryptonella 1
Navicula decussis 21
Navicula dicephala 21
Navicula disculus 2
Navicula elginense 1
Navicula gastrum 11
Navicula gracilis 1
Navicula gregaria 1
Navicula halophila 7
Navicula hasta 16

Navicul hungaric 5
Navicula cqryptocephala v. intermedia 1
Navicula jaernefeltii 2
Navqicula lacustris 1
Navicula laevissqima 17
Navicula leptostriata 3
Navicula lucinensqis 1
Navicula capitata v. lueneburgensis 2
Navicula menisculus 2
Navicula minima 2
Navicula placenta 4
Navicula placentula 6
Navicula protracta 4
Navicula psuedoscutifoxmis 6
Navicula pupula 41
Navicula radiosa 20
Navqicula rhyncocephala 10
Navicula salsa 3
Navicula subplacentula 1
Navicula subqrhyncocephala 1
Navicula schroeteri 11
Navicula scutelloides 2
Navicula sp. 5 1
Navicula sp. 6 1
Navicula sp. 7 1
Nqavicula sp. 8 1
Navicula sp. 9 1
Navicula sp. 10 1
Navicula sp. 2
Navicula scutiformis 2
Navicula stroemli 1
Navicula subhamulata 1
Navicula tanera 2
Navicula trqivqialis 4
Navicula tuscula 2
Navicula viridula 66
Navicula radiosa v. tenella 1
Navicula yarrensis 1
Navicula yecens 1
Neidium affine 19
Neidium affinis v. amphyrineus 1
Neidium ampliatum 2
Neidium binode 1
Neidium densestriatum 1
Neidium dilatatum 2
Neidium dubium 6
Neidium, iridis 12
Neidium productum 5
Pinnularia acrosphaeria 1
Pinnularia acuminata 1
Pinnularia borealis 3
Pinnularia braunii 2
Pinnularia divergens 61
Pinnularia gibba 28
Pinnularia legumen 4
Pinnularia major 21
Pinnularia microstauron 5
Pinnularia obscura 2
Pinnularia sp. 2 81
Pinnularia sp. 3 81

Pinnularia subcapitata 4
Pinnularia sudetica 5
Pinnularia viridis 12
Stauroneis agrestris 1
Stauroneis anceps 17
Stauroneis anceps f. gracilis 3
Stauroneis nobilis 1
Stauroneis phoenicenteron 17
Stauroneis prominula 1
Stauroneis schqimanskii 1
Stauroneis anceps v. siberica 1
Stauroneis smithii 16
Stauroneis sp. 2 1
Stauroneis sp. 3 1
Tropidoneis lepidoptera 3
Family ..... Epithemiaceae
Epithemia zebra v. porcellum 1
Epithemia zebra 12
Rhopalodia gibba 2
Rhopalodia g-tbberula 1
Family ..... Nitzschiaceae
Bacillaria paxillifer 28
Denticula sp. 1
Denticula thermalis 1
Hantzschia amphioxys 1
Hantzschia virgata v. capitellata 3
Hantzschia virgata 8
Nitzschia acicularis 18
Nitzschia acuta 4
Nitzschia amphibia 3
Nitzschia acicularis v. closterioides 2
Nitzschia communis 2
Nitzschia closterium 1
Nitzschia dissipata 6
Nitzschia dubia 2
Nitzschqla frugalis 3
Nitzschia gracilis 8
Nitzschia hantzschiana 3
Nitzschia tryblionella v. laevidensis 4
Nitzschia linearis 1
Nitzschia tryblionella v. levidensis 2
Nitzschia palaecea 3
Nitzschia palea 21
Nitzschia parvula 1
Nitzschia romana 12
Nitzschia rostellata 1
Nitzschia sigmoidea 6
Nitzschia sp. 3 2
Nitzschia sp. 4 21
Nitzschia sp. 5 2
Nitzschia sp. 6 2
Nitzschia sp. 7 21
Nitzschia tryblionella v. subsalina 61
Nitzschia triblionella 24
Nitzschia tryblionella v. victoriae 4
Nitzschia vitrea-like 01
Family ..... Surirellaceae,
Campylodiscus sp. 21
Cymatopleura solea 2
Stenopterobia intermedia 2

Surirella angustata 5
Surirella biseriata 6
Surirella elegans 3
Surirella gracilis 4
Surirella linearis 16
Surirella ovata 5
Surirella robusta 15
Surirella tenera 59
Order ...... Centrales
,Suborder ... Coscinodiscineae
Family ..... Thalassiosiraceae
Aulacosira granulata 16
Cyclotella meneghiniana 21
Cyclotella stelligera 1
Cyclotella striata 6
Thalassiosira decipiens 1
Thalassiosi.ra eccentrica 1
Thalassiosira sp. 1 1
Thalassiosira sp. 2 1
Family ..... Melosiraceae
Melosira italica 1
Melosira undulata 35
Melosira varians 31
Paralia sulcata 1
Suborder ... Biddulphiineae
Family ..... Biddulphiaceae
Hydrosera triquetia 2
Terpsinoe americana 2
Tezpsinoe musica 3
Division ... Chlorophyta. -
Class ...... Chlorophyceae (green algae)
or-der ...... Chaetophorales
Family ..... Chaetophoraceae
Chaetophora-like form 1
Or-der ...... Chlorococcales
Family ..... Hydrodictyaceae
Pediastrum duplex 1
Pediastrum simplex 2
Family... i.Scenedesmaceae
Scenedesmus sp. 252 1
Scenedesmus armatus 6
Scenedesmus dimorphus 12
Scenedesmus obliquus 3
Tetraedron trigonium v. gracile 1
Order ...... Volvocales
Family ..... Volvocaceae
Pandorina morum 3
Order ...... Zygnemales
Family ..... Desmediaceae
Arthrodesmus octocorne 2
Arthrodesmus subulatus 1
Arthrodesmus triangularis v. 1
Bambusina brebissonii 2
Closterium bailyanum 4
Closterium libellula 3
Closterium sp. 1 3
Closterium sp. 2 1
Closterium sp. 3 2
Closterium sp. 4 3

Closterium sp. 5 (giant one r254/29) 1
Cosmarium contractum 1
Cosmarium punctulatum 1
Cosmarium sp. 1 1
Cosmarium sp. 2 (254) 1
Cylindrocystis americana 1
Desmidium aptogonum 1
Docidium undulatum 1
Euastrum affine 1
Euastrum gemmatwn 1
Gonatozygon pilosum 1
Gymnozyga moniliformis 1
Penium sp. 1
Staurastrum cornatum 2
Staurastrum limneticum v. coqrnutum 1
Staurastrum curvatum 2
Staurastrum paradoxum 3
Staurastrum cornatum s. coqrnatum 1
Staurastrum sp. 1 1
Tetmemorus breqbqissonii 2
Tetmemorus granulatus 1
Family ..... Zygnemaceae
Mougeotia elongatula 1
Mougeotia sp. 1 (narrow trichomes) 2
Mougeotia sp. 2 (wide trichomes) 2
Mougeotia sp. 3 1

Species richness in the main stream was comparable to that in the various

tributaries. -rhe species richness in most of the river statioris was considerably

higher than that in the estuary. The data indicate that main stream

phytoplankton abundance and species richness showed relative stereotypic

distributions in terms of the overall habitat characteristics in the river-estuarine

system. The uniformly high numbers of phytoplankton in the productive estuary
throughout -the year was in contrast to the more seasonal phytoplankton

abundance in the river. Areas of high flow were characterized by low numbers

of individuals; species richness in the main stem, however, was comparable to
the tributariE)s. The salinity-stressed estuarine conditions could be associated
with the low species richness in the eastern portion of Choctawhatchee Bay.

In terms of species richness at most of the river stations, there was a

general pattern of high numbers of species during January, 1987 followed by a

decline during the succeeding months with or without a second peak during the
fall. Overall species richness for a given month was highest in Holmes Creek.

Species richness patterns in the estuary were quite variable from station to

station. At station 15, there were peaks during late spring and winter months.

At stations 3 and 7, such peaks tended to occur during spring and summer

months. In terms of numerical abundance, there was considerable station to

station variability. In general, there were winter-spring and fall peaks of

abundance, but such peaks followed station -specific patterns over the period of

observation. The high numbers of phytoplankton in Pine Log Creek (due to the
February b1loom) and Holmes Creek (again, a February bloom contributed

heavily to the observed winter peak) are evident in contrast to the very low

numbers of phytoplankton taken at the upper Choctawhatchee River station and

in Bruce Creek and Sandy Creek. The biomass trends followed the numerical

trends closely. When viewed as mean numbers of species (cumulative species

richness), another pattern is evident. The,lowest phytoplankton mean species

richness occurred in Seven Mile Creek (62) followed closely by Bruce Creek

(64) and the upper Choctawhatchee River (70). The highest mean species

richness of phytoplankton in the Choctawhatchee system occurred in Pine Log

Creek (60) and Sandy Creek. The other main stem stations and larger Creeks

(Holmes, Wright's) had intermediate levels of cumulative species richness.

Over the period of study, the main channel stations (70,68,61) had

relatively high species-specific dominance with 6-8 species accounting for the

overall numorical abundance of phytoplankton over the year of study. A group

of 7-13 sub-dominant species were present followed in order of abundance by

a considerable number of species with low numbers taken over the study

period. Species such as Achanthes lanceolata v. dubia and v. apiculata,

Navicula s,pp, Surirella tenera, and Synedra ulna were usually the top

dominants at the main (channel) stations. Overall (cumulative) totals of the

numbers of species for the year tended to increase downstream (station 70, 81;

station 68, 100; station 61, 101).

In Wright's Creek (station 69), the dominance patterns in terms of
numbers of individual species populations tended to follow that described at the

main river stations. There were some differences in the sub-dominant species.

The cumulative total number of species in Wright's Creek was 114. In Holmes

Creek (station 65), dominance hierarchies were quite different than those

described above. Top dominants included species such as Achnanthes clevei,
Cocconeis placentula and C. dimunuta, Eunotia pectinalis, Fragilaria

constuensh;, and the Achnanthes spp. There was a cumulative total of 128

species in Holmes Creek. In Sandy Creek (station 67), the top dominants were

fewer in nurr@,iber although the species strongly resemble those described for the

main river stations and Wright's Creek. The numbers were quite low in this

creek and the cumulative species total was 112, similar to that in Wright's

Creek. Bruce Creek (station 64) showed a somewhat different pattern with a
single top dominant, Eunotia pectinalis, followed by a series of 11 sub-

dominants that resembled the species lists described above for the various

main channel stations. The cumulative total of 123 species was on the high

side resembling that of Holmes Creek.

In Seven Run Creek (station 62), the pattern of species abundance

resembled that described for Bruce Creek with Eunotia pectinalis as the top

dominant followed by a series of sub-dominants composed of species similar to

those described above for the various other stations. Once again, numbers of

species were relatively low in this creek, with a cumulative total of only 94

species. In Pine Log Creek, the dominance pattern followed that described for

Bruce Creek and Seven Run Creek. A cumulative total of 145 species at this

station was the highest such number found in the survey. The phytoplankton

data in Pine! Log Creek (station 60) indicate a similar pattern to that described

for some of -the tributaries. Eunotia pectinalis was the top dominant followed by

a group of sub-dominants that included most of the familiar species listed as

sub-dominants at the various other river stations. The numbers at this station

were perio6cally high so that substantial totals were noted for Achnanthes spp,

Frustulia r@omboides, Navicula spp, and Eunotia alpina. The cumulative
species richness at the various river stations follows a pattern that is similar to
though not identical with the mean species numbers (means of the numbers of
species per sample). The cumulative species number was highest at Pine Log

Chaetoceros spp. The high numbers of phytoplankton per month were

accompanied by a relatively low cumulative number of species (92). At station

7, the top dominant was the same as that described at station 3; the sub-

dominants were similar in terms of species and distribution although the exact

order within the dominance hierarchy was somewhat different. Overall numbers

were substantially higher at station 7; the cumulative species richness was 97.

At station 15, the numbers were higher still with the top dominant being

Cyclotella striata. The sub-dominants were somewhat different in terms of

species than those described above. The cumulative species richness of 87

was relatively low. Thus, compared, with the river stations, the estuarine areas

had higher numbers of phytoplankton though lower cumulative species
richness than the river statioris. Dominance was similar among the various bay

stations although the species noted were quite different from those observed at

the river stations.

B. Estuarine phytoplankton distribUtion

1. Wetter quality

A summary review of water quality is given in Figure 2. A detailed
analysis of these data is given in Livingston (1986a). Salinity in the
Choctawhatchee Bay system is lowest in eastern sections due to river input and
in the northern bayous. Salinity was high in Old Pass Lagoon. Peak salinities
occurred in the bay during the months of July through October. Vertical salinity
stratification occurs in various portions of the estuary during certain months.

Such stratiCcation is evident in the vertical dissolved oxygen distribution that

occurs in the bay during warm months. Deep stations throughout the bay had

CHOCTAWHATCHEE BAY
Salinify in ppf
Average Surface Samples For All Dafes

CHOCTAWHATCHEE BAY
Salinity in ppf
Average Boffom Samples For All Dafes

-t ell,

CHOCTAWHATCHEE BAY
Dissolved Oxygen in ppm
Average Surface Samples For All Dafes

7@) ),rl

CHOCTAWHATCHEE BAY
Dissolved Oxygen in pprn
Average Bottom Samples For All Dates

CHOCTAWHATCHEE BAY
Turbidify in NTU
Average Surface Samples For All Dafes

AL EO

%.I.HUU I AWHAI'CH'EE BAY
Turbidity in NTU
Average Bottom Samples For All Dates

Ilk

CHOCTAWHATCHEE BAY
Color in Pf-Co Unifs
Average Surface Samples For All Dafes

N I

-@f'A L EO

CHOCTAWHATCHEE BAY
Color in Pf-Co Unifs
Average Boftom Samples For All Dafes

S CYI.,

CHOCTAWHATCHEE BAY'
Depth in Meters
Average of All Sample -Dates

Ilk

CHOCTAWHATCHEE BAY
Secchi Readings in Meters
Averar, A I Z@
ge of "ll Sample Dates

CHOCTAWHATCHEE BAY
Total Nitrogen in Milligrams Per Liter
ANIOrrTria r%f qivrf)@ir-= IIZrirnr%I.=c Pr%r All r/)ri+PQ

Ilk

CHOCTAWHATCHEE BAY
Total Kjelclahl Nitrogen in Milligrams Per Liter
Average of Bottom Samples For All Dates

-49

CHOCTAWHATCHEE BAY
Ortho-phosphate in Milligrams Per Liter
Average of Bottom Samples For All Dates

Ilk

CHOCTAWHATCHEE BAY
Tofal Phosphafe in Milligrams Per Lifer
Average of Surface Samples For All Dafes

-/0 0

CHOCTAWHATCHEE BAY
Ammonia in Milligrams Per Lifer
Average of Surface Samples For All Dafes

C"HOCTAWHATCHEE BAY
Ammonia in Milligrams Per Liter
Average of Bottom Samples For All Dates

CHOCTAWHATCHEE BAY
Nitrite in Milligrams Per Liter-
Average of Surface Samples For All Dates

CHOCTAWHATCHEE BAY
Nitrite in Milligrams Per Liter
Average of Bottom Samples For All Dates

-/0 0 Q 00@

CHOCTAWHATCHEE BAY
Nitrate in,Milligrarns Per Liter
Average of Surface Samples For All Dates

CHOCTAWHATCH-EE BAY
Nitrafe in Milligrams Per Lifer
Average of Bottom Samples For All Dates

-60

CHOCTAWHATCHEE BAY
Total Kjeldahl Nitrogen in Milligrams Per Liter
Average of Surface Samples For All Dafes

CO"HOCTAWHATCHEE BAY
Toi-al Nifrogen in Milligrams Per Lifer
Average of Bottom Samples For All Dates

0 -k b 6@

C'HOCTAWHATCHEE BAY
Ortho-phosphate in Milligrams Per Liter
t
Average of Surface Samples For All Dafes

CHOCTAWHATCHEE BAY
Tofal Phosphafe in Milligrams Per Lifer
Average of Bottom Samples For All Dates

CHOCTAWHATCHEE BAY
Ratio of Total Phosphate to Total Nitrogen
Average of Surface Samples For All Daf es

0 40
00/

CHOCTAWHAT .CHEE BAY
Ratio of Total Phosphate to Total Nitrogen
Average of Bottom Samples For All Dates

4;p

o -jb 6y OC),(

low dissolved oxygen at various seasons of the year. Areas of particularly low

D. 0. included lower Rocky Bayou, Boggy Bayou, Tom's Bayou, Garnier Bayou,

Cinco Bayou, and Old Pass Lagoon.

Turbidity and color followed similar east-west gradients with the highesL
levels in areas proximal to the entry point of the Choctawhatchee River.

Relatively high color was also noted in some of the northern bayous during the

period from December through March. Such factors were inversely related to

Secchi depth readings. Overall, the vertical stratification of the Choctawhatchee

estuary follows seasonal changes of temperature and salinity. In the late

summer, hypoxic conditions are widespread throughout the bay at depth which

is an important water quality condition in the system.

Ammonia levels were highest at depth in mid-sections and western

portions of the bay. Such concentrations were highest during September and
October. Nitrite-N and total N levels were lowest in mid-po-rtions and

northeastern sections of the estuary. Nitrate-N was highest in western areas.

Peaknitrogen levels occurred -during winter months. Orthophosphate was

highest in peripheral stations in eastern and western sections of the bay. Mean
bottom orthophosphate -was high in Old Pass Lagoon (station 36E), peaking
during fall months. Average total phosporous was particularly high in Old Pass

Lagoon where the P/N ratios were also high. This area of bay has been

described in d etail by Livingston (1986b). This area is poorly flushed and

receives ahthropogenous contamination from urban areas and a marina.

Nitrogen and phorphorous nutrients and particulate organic matter (POM) were

higher in Old Pass Lagoon than in other portions of the bay and such

differences were shown in an ordering of the data (Table 2). Cultural

eutrophication was evident in the increased numbers. of phytoplankton in Old

Pass Lagoon. This basin was also hypoxic at depth, especially in eastern

surtace ancl oottom station ciata pootea).

N02,NO3,TKN CLUSTER - ALL DATES, TOP I BOTTOM

CLUSTERING STRATEGY IS FLEXIBLE GROUPING (WITH BETA)
SIMILARITY COEFFICIENT IS CZEKANOWSKI

CLUSTER GROUP WITH (WHERE GROUP NAME NOW REFERS TO A CLUSTER
LEVEL JOINS NAME SUBGROUP CONTAINING THE FOLLOWING CLUSTER UNITS)

'9810
27 -33 27 33

.9808 34 36E 34 36E

.9656 27 34 27 33 34 36E

.9584 32 37 32 37

..9253 36W 39 36W 39

.9057 27 38 27 33 34 36E 38

.8926 27 31 .27 31 33 34 36E 38

.8851 32 35 32 35 37

.7177 27 36W 27 31 33 34 36E 36W 38 39

.6072 32 44 32 35 37 44

.3084 27 32 27 31 32 33 34 35 36E 36W
37 38 39 44
(ALL ONE GROUP)

N02vNO3qTKN CLUSTER ALL DATESP TOP BOTTOM AVERAGED
DENDROGRAM OUTPUT
MINIMUM DISTANCE .3084

1.0 .9 .8 .7 .6 .5 .4 .3 .2 .1 .0

33 --- *I
I
34 --- *I I
I* I-*
36E I I
I I----------------
38 ---------- * I
I
31 ------------- ----------------------------------------

36W --------
I --------------------
39 --------

32 -----

37 ----- I---------------------------
I
35 ------------ -1 -----------------------------

OR'lHO AND TOTAL PHOSPHATE - ALL DATESP T & B POOLED
CLUSTERING STRATEGY IS FLEXIBLE GROUPING (WiTH BETA)
SIMILARITY COEFFICIENT IS CZEKANOWSKI

CLUSTER GROUP WITH (WHERE GROUP NAME NOW REFERS TO A CLUSTER
LEVEL JOINS NAME SUBGROUP CONTAINING THE FOLLOWING CLUSTER UNITS)

.9640 31 33 31 33

.9305 37 39 37 39

.9128 27 37 27 37 39

..9026 32 34 32 34

.8550 27 38 27 37 38 39

.8496 35 44 35 44

.8370 36E 36W 36E 36W

.7134 27 32 27 32 34 37 38 39

.4357 27 31 27 31 32 33 34 37 38 39

.1119 27 36E 27 31 32 33 34 36E 36W 37
38 39

-.2457 27 35 27 31 32 33 34 35 36E 36W
37 38 39 44
(ALL ONE GROUP)

ORTHO AND TOTAL PHOSPHATE ALL DATESP T I B POOLED
DENDROGRAM OUTPUT
MINIMUM DISTANCE = -.2457

1.0 .8 .6 .4 .2 .0 2 -.4 -.6 -.8 -1.0

27 -----

37 ---- *I I

38 -------- I-------------
I
32 ------ z I
---------------
34 ------

31 --- I
I ------------------------- I-----------------
33 --- I I
I I
36E --------- I I
I-----------------------------------
36W ---------

35 ---------
I-----------------------------------------------------
44 ---------

CLUSTERING STRATEGY IS FLEXIBLE GROUPING (WITH BETA)
SIMILARITY COEFFICIENT IS CZEKANOWSKI

CLUSTER GROUP WITH (WHERE GROUP NAME NOW REFERS TO A CLUSTER
LEVEL JOINS NAME SUBGROUP CONTAINING THE FOLLOWING CLUSTER UNITS)

.9975 27 34 27 34

.9945 33 38 33 3B

.9848 31 37 31 37

.9714 27 35 .27 34 35

.9686 44 36E 44 36E

.9550 32 33 32 33 38

.9281 27 39 27 34 35 39

.9141 31 32 31 32 33 -37 38

.8524 44 36W 44 36E 36W

.6134 27 31 27 31 32 33 34 35 37 38
39
.0760 27 44 27 31 32 33 34 35 37 38
39 44 36E 36W
(ALL ONE GROUP)

PARTICULATE ORGANIC MATTER (SEP 85 FEB 86) SURFACE I BOTTOM AVERAGED
DENDROGRAM OUTPUT
MINIMUM DISTANCE .0760

1.0 .9 .8 .7 .6 .5 .4 .3 .2 .1 .0

34 1---
I
35 ---- I -------------------------------
I
39 ------
----------------------------------------------------
31 ---

37 ---
I-----------------------------
32 ----- I

44 ----
I-----------
36E ---- ----------------------------------------------------------------------------

36W ----------------

SURFACE PHYTOPLANKTON COUNTS (SEP 85 - JAN 86)

CLUSTERING STRATEGY IS FLEXIBLE GROUPING (WITH BETA)
SIMILARITY COEFFICIENT IS CZEKANOWSKI

CLUSTER GROUP WITH (WHERE GROUP NAME NOW REFERS TO A CLUSTER
LEVEL JOINS NAME SUBGROUP CONTAINING THE FOLLOWING CLUSTER UNITS)

.8723 34 38 34 38

.5057 31 34 31 34 38

.2719 31 36 .31 34 36 38
(ALL ONE GROUP)

SURFACE PHYTOPLANKTON COUNTS (SEP 85 JAN 86)
DENDROGRAM OUTPUT
MINIMUM DISTANCE .2719

1.0 .9 .8 .7 .6 .5 .4 .3 .2 .1 .0

31 --------- ---------------------------------------
I-----------------------
34 -------------- * I
I-----------------------------------
38 --------------

36 --------------------------------------------------------------------------

sections of the lagoon. According to Livingston (1987), water and sediments in
the Choctawhatchee estuary were relatiyely clear of a-'broad spectrum of

organic compounds such as organochlorine pesticides, polychlorinated

biphenyls, dioxin, organophosphorous pesticides, and chlorinated herbicides.

Eastern and central portions @of the estuary had relatively high metal

concen trations in the sediments which also had high silt/clay fractions. High

metal concentrations were also found in the urbanized bayous in the western

section of the bay (Boggy, lower Rocky, Garnier, Old Pass Lagoon) with

stormwater runoff and marinas as the most likely sources of pollutants. Infaunal

macroinvertebrate associations indicated degraded conditions in Old Pass
Lagoon which--had high leve Is-("e n rich ed" as defined by FIDER guidelines) of

cadmium, copper, lead, and zinc in the sediments (Table 3).
Chlorophyll a (Figure 3) was found in the highest concentrations in

eastern portions of the bay. Particulate organic matter was highest in Old Pass

Lagoon and some of the eastern bay stations (Figure 4).

2. Taxonomic review: s .pecies occurrence

The highest overall numbers of phytoplankton were noted in Old Pass

Lagoon and the westernmost sampling station (Figure 5). These stations were

also highest in phytoplankton species richness. Such data indicate that the

nutrient-enriched waters of the western bay stations that receive stormwater

runoff from urbanized areas and/or are the sites for major marinas are subject to

major increases in phytoplankton numbers. However, such high concentrations

could also be due, in part, t o reduced predation due to low numbers of

zooplankton in addition to the more obvious correlation with high nutrient levels

(Figure 6). Overall, the general distribution of phytoplankton in the bay indicates

Table 3: Metal" accumulation Index (A) computed for seven metals
at 25 locations sampled in sediments of Choctawhatchee Bay
In April, 1987.

TA IArsenic lCadmium Copper lphro-miuml Lead I Nickel Zinc
01 20.561 0.93 1.59 0.74 1.32 0.83 1.27
03 5.002 1.60 4.472 2.74 1.42 2.402 1.81
05 4.871 2.48 5.821 0.77 2.091 1.43 1.61
.07 2.00 1.42 5.042 2.87 1.22 2.672 1.96
0 9 3.69 0.93 0.92 0.78 2.031 0.38 0.89
11 5.212 1.00 5-.032 2.77 1.32 2.502 1.81
13 6.222 3.27 2.64 3.202 2.692 2.03 1.67
15 3.00 1.10 1.63 1.88 1.35 1.35 1.26
17 5.241 0.36 2.18 .2.32 1.94 1.83- 1.33
19 7.252 1.69 7.642 3.632 1.77 4.652 2.422
20 1.62 0.38 0.57 0.92 1.56 0.76 0.78
25 5.412 1.01 2.74 2.35 1.70 2.392 1.60 -
6 B 4.911 2.41 3.041 1.16 2.221 2.341 1.89
27 0.57 1.02 1.29 0.87 2.541 0.93 1.25
28 1.28 2.21 2.911 2.16 2.611 2.581 1.70 -
29 .1.82 4.811 3.701 3.791 4.571 2.941- 2.351
30 3.45 10.351 1.90 1.56 2.501 0.97 1.59 -
31 5.771 1.55 5.751 0.92 2.441 2.391 1.71
32 0.90 1.58 1.12 0.90 1.99 0.70 1.21
34 3.21 3.05 2.33 2.02 2.231 2.19 1.73
6E 2.37 5.211 13.361 1.93 9.291 1.55 11.171
37 18-831 0.94 0.97 0.88 6.011 0.77 1.01
38 3.26 0.34 0.48 0.49 3.211 0.78 1.02
40 1.99 4.881 3.921 2.96 5.911 2.821 3.041
42 1 0.84 0.91 1.70 0.65 3.741 0.70 1 2.21

metal enriched at this station

metal possibly enriched at this station (aluminum concentration > 79,000 ppm
precludes assignment as enriched)

througii AU6Ubt, k VkOV.

CHOCTAWHATCHEE BAY
Chlorophyll a in Milligrams Per Cubic Meter
Average of Surface Samples For All Dates

CHOCTAWHATCHEE BAY
Chlorophyll a in Milligrams Per Cubic Mefer
Average of Boffom Samples For All Dafes

zq@

J, 63

September, 1985 through August, 1986.
CHOCTAWHATCHEE BAY
Parficulate Organic Maffer in Milligrams Per Lifer
Average of Surface Samples For All Daies

CHOCTAWHATCHEE BAY
Particulate Organic Matter in Milligrams Per Liter
Average of Bottom Samples For All Dates

Ikk

Ilk :@k

Figure 5: Summary data (12 m onth averages) -.'phytoplankton
numbers and species richness taken during the day in the
Choctawhatchee Say system from September, 1985 through
August, 1986.

CHOCTAWHATCHEE BAY
Phytoplankton in Number of Individua Is Per Cubic Meter
Average of Day Surface Samples For All Dates

24, 00 o66
lvo'ooo

CHOCTAWHATCHEE BAY
Phytoplankton in Number of Species
Average of Day Surface Samples For All Dates

-fo

Figure 6: Summary data (12 month averages) of physical-chemical
taken in the Choctawhatchee Bay system from September,
1985 through August, 1986.

CHOCTAWHATCHEE BAY
Zooplankton in Number of Individuals Per Cubic Meter
Average of Day Surface Samples For All Dates

'ao

CHOCTAWHATCHEE BAY
Zooplankton in Number of Species
Average of Day Surface Samples For All Dates

a positive (direct) relationship with areas enriched by chemicals associated with

anthropogenous activities.

A review of the spatial/temporal occurrence frequency of estuarine algae

in Choctawhatchee. Bay is given in Table 4. Two genera were dominant in terms

of the numbers of species: Navicula and Nitzschia. In terms of the most
frequently taken species, there was a series of dominants: Ceratium hircus,

Cyclotella striata, Cyclotella sp., Chaetoceros decipiens, C. radicans, C. brevis,

Coscinodiscus centrafis, and C. granfi. Of these species, a group of dominants
was chosen for an analysis of distribution along specific habitat gradients. Such

species (16) were chosen as frequency dominants (occurring during all times of

the year) or as numerical dominants ( the top species in terms of numbers taken

over the entire sampling period). It can be argued that sub-dominant and rare

species can be important indicators of water quality. However, for the purposes

of this study, only the dominants were treated as a function of water quality

factors that include salinity, dissolved oxygen, and various nutrients.

3. Algae as water quality indicators

Numbers of individuals, numbers of species, and the Shannon diversity

index were used as phytoplankton community indices. The data (Figure 7)
indicate that the station in the western section of the bay that was characterized

by high nutrient levels (36E) was also characterized by periodic peaks of

phytoplankton numbers (in this case, the late fall and early winter months).
Relatively high numbers of phytoplankton were also found at station 38 which
was subject to stormwater runoff from urbanized areas of the western portions of
the bay. Species richness was also high at the eutrophicated stations. Old pass
lagoon had relatively high species richness during most of the year with low

Table 4: Systematic review of phytoplankton taken with 25 and 64
gm nets in the Choctawhatchee estuary from September,
1985 through August, 1986.

Systematic review

Choctawhatchee Bay, day, surface,. 25g sanples

No. of occurrences
Division ... Cyanophyta
Class ...... Cyanophyceae (blue-green algae or cyanobacteria)
Order ...... Chroococcales
Family ..... Chroococcaceae
Synechocystis sp.
Order ...... Nostocales
Family ..... Nostocaceae
Anabaena sp.
Family ..... Oscillatoriacea6
Oscillatoria sp. 3 1.
Division...Euglenophyta
Class ...... Euglenophyceae
Order ...... Euglenales
Phacus sp.
Division-Cryptophyta
Class ...... Cryptophyceae
Order ...... Crytopmonadales
Family ..... Crytomonadaceae
Cryptomonas sp. 1 3
Ctyptomonas sp. 1
Division ... Dinophyta
Class ....... Dinophyceae (dinoflagellates)
Unidentified dinoflagellates 1
Order ...... Peridiniales
Family ..... Peridiniaceae
Peridinium oblong= 2
Peridinium sp. 1
Order ...... Gonyaulacales
Family ..... Ceratiaceae
Ceratium fusus 3
Ceratium hircus 19
Ceratium tripos 1
Family ..... Gonyaulacaceae
Gon_Vaulax sp. 1 5
Order ...... Prorocentrales
Family ..... Prorocentraceae
Prorocentrum qracile 1
Prorocentrum micans 13
Pronoctiluca acuta 1
Prorocentrum pyriformis 1
Prorocentrum sp . 1 1
Pz-orocentrum triestinum I
Division ... Chrysophyta
Class ...... Chrysophyceae (golden-brown algae)
Order.... Chrysomonadales
Family ..... Ochromonadaceae
Dinobryon divergens 1
Dinobryon sertularia 2
Division ... Xanthophyta
Class ...... Xanthophyceae (yellow-green algae)

Order ...... Triboemales
Family ..... Tibonemataceae
Tribonema affine 3
Division ... Bacillariophyta (diatoms)
Class ...... Bacillariophyceae
Order ...... Pennales
Suborder ... Araphidineae
Family ..... Diatomaceae
Asterionella japonica 2
Ctenophora pulchella 1
Delphinels surirella 3
Falcula hyalina 4
opephora martyi 2
Opephora pacifica 4
Rhabdonema adriaticum 8
Synedra acus 5
Synedra sp. q1
Synedra ulna 8.
Thalassionema nitzschioides 9
Thalassiothrix longissima 1
Suborder ... Raphidinede
Family ..... Eunotiaceae
Eunotia alpqina 3
Eunotia pectinalis 5
Eunotia serra 1
Family ..... Achnanthaceae
Cocconeis placentula 7
Cocconeis pseudomarginata 1
Cocconeis scutellum 1
Family ..... iaviculaceae
Amphiprora gigantea 9
Amphora coffeaefozmis 2
Amphora commutata 1
Amphora ovalis 1
Caloneis acutiascula 2
Caloneis formosa 2
Caloneis latiascula (new var cr 249) 1
Caloneis latiascula 5
Caloneis permagna 1
Caloneis westii 1
partogramma crucicula 2
Cymbella gracilis 1
Diploneis elliptica 1
Diploneis ovalis 5
Diploneis parma 1
Diploneis sp., 1 1
Frustulia rhomboides 2
Gomphonema angustatum 3
Gomphonema gracile 21
Gyrosigma acuminatum 61
G sigma macrum I
Y0ro
Gyros0qigma spenceri 61
Navicula cf. ammophila 4
Navicula bailyana 21
Navicula distans 2
Navicula longa 61
Navicula yra 6
Navicula pupula 2
Navicula salsa 2

Navicula sp. 1 1
Navicula viridula 2
Navicula yarrensis v. americana 1
Navicula yarrensis 14
Neidium iridqis 1
Pinnularia gibba 1
Pleurosigma elongatum 4
Pleurosigma sp. 2
Stauroneis phoenicenteron 2
Stauroneis spicula 4
Tropidoneis lepidoptera 2
Family..... Nitzschiaceae
Bacillaria paxillifer 12
Nitzschia circumsuta 1
Nitzschia acicularis v. closterioides 10
Nitzschia constricta 2
Nitzschia dubia 1
Nitzschia jelinecki 1
Nitzschia lanceolata I
Nitzschia linearis 2
Nitzschia longissima 9
Nitzschia sp. (needle-like) 1
Nitzschia sigma 3
Nitzschia sigmoidea 6
Nitzschia triblionella 7
Family..... Surirellaceae
Surirella fastuosa 12
Surirella gemma 5
Surirella ovata 2
Surirella robusta 1
Order...... Centrales
Suborder...Coscinodiscineae
Family..... Thalassiosiraceae
Aulacosira granulata 2
Cyclotella meneghiniana 1
CYclotella sp. (small) 18
Cyclotella stelligera 1
Cyclotella striata 33
Cyclotella stylorum 7
Skeletonema costatum 7
Thalassiosira decipiens 2
Thalassiosira eccentrica 13
Thalassiosira lineatus 1
Thalassiosira oestrupii 15
Family.....Melosiraceae
Leptopylindrus danicus 5
Melosira granulata 1
Melosira undulata 2
Melosira varians 3
Paralia sulcata 5
Podosira stelliger 1
Family.....Hemidiscaceae
Actinocyclus ehrenbergii 1
Family.....Heliopeltaceae
Actinoptychus undulatus 8
Family.....Eupodiscaceae
Triceratium arcticum 1
Family.....Chaetoceraceae
Bacteriastrum varians 1
Chaetoceros atlanticus 4

Chaetoceros brevis 19
Chaetoceros compressus 2
Chaetoceros costatum 1
Chaetoceros decipiens 18
Chaetoceros didymus 14
Chaetoceros eibonii 2
Chaetoceros lauderi 5
Chaetoceros messanensis 6
Chaetoceros socialls 3
Family ..... Rhizosoleniac eae
Rhizosolenia alata 5
Rhizosolenia delicatula 1
Rhizosolenia fragilissima 3
Rhizosolenia imbricata 1
Rhizosolenia setigera 1
Rhizosolenia sp. 1
Rhizosolenia stolterfothii 9
Family ..... Coscinodiscaceae
Coscinodiscus centralis 17
Coscinodiscus granil 5
Suborder ... Biddulphiineae
Family .... Biddulphiaceae
Hemiaulus centralis 3
Hemiaulus sinensis 1
Division ... Chlorophyta
Class ...... Chlorophyceae (green algae)
Order ...... Chlorococcales
Family ..... Hydrodictyaceae
Pediastrum simplex 1
Family ..... Oocystaceae
Kirchneriella subsolitaria 1
Family ..... Scenedesmaceae.
Scenedesmus dimorphus 2
Order ...... Volvocales
Unidentified green flagellates 1
Family ..... Pyramimonadaceae
Pyramimonas sp. 1 4
Order ...... Zygnemales
Family ..... Desmediaceae
Stauqrastrum paradoxum 1
Family ..... Zygnemaceae
Mougeptia sp. 1 (narrow trichomes) 1

Systematic review

Choctawhatchee Bay, day, surface, 64u samples

No. of occurrences
Division...Cyanophyta
Class ...... Cyanophyceae (blue-green algae or cyanobacteria)
Order ...... Chroococcales
Family ..... Chroococcaceae
Merismopedia aeruginea 1
Merismodedia elegans 1
Merismopedia thermale 1
Synechococcus sp. 2
Order ...... Nostocales
Family ..... Nostocaceae
Anabaena cylindrica 1
Anabaena inaequalis 8
Anabaena sp. 1 2
Anabaena sp. 2 1
Anabaena sp. 4
Anabaena variabilis 2
Family ..... Oscillatoriaceae Hydorcoeleum lyngbyaceum 1
Johannesbaptistica sp. 2
Lyngbya sordida 2
Microcoleus lyngbyaceus 1
Oscillatoria sp.3 2
Oscillatoria tenuis 1

Division...Dinophyta
Class ...... Dinophyceae (dinoflagellates)
Unidentified dinoflagellates- 4
Order ...... Gymnodiniales
Family ..... Gymnodiniaceae
Amphidinium carteri 3
Amphidinium sp. 2
Gymnodinium coeruleum 1
Gymnodinium sp. 1 1
Gymnodinium sp. 3
Family ..... Polykrikaceae
Polykrikos sp. 2
Order ...... Peridiniales
Family ..... Peridiniaceae
Oxyhris marina 1
Peridinium brochii 1
Peridinium claudicans 4
Peridinium conicum 1
Peridinium crassipes 12
Peridinium depressum 2
Peridinium divergens 3
Peridinium elegans 1
Peridinium gracile 2
Peridinium leonis 3
Peridinium oblongum 16
Perldinium sp. 6
Peridinium venustum 1
Family ..... Protoperidiniaceae

Diplopsalis lenticula 1
Diplopsalis sp. 8
Encysted dinoflagellate 55
order ...... Dinophysiales
Family ..... Amphisoleniaceae
Amphisolenia sp. 1
Family ..... Dinophysiaceae
Dinophysis caudata f. acutiformis 12
Dinophysis caudata 18
Dinophysis ovum 1
Dinophysis caudata v. pedunculata 15
Ornithoceros sp. 3

order ...... Gonyaulacales
Family ..... Ceratiaceae
Ceratium tripos v. atianticum 11
Ceratium carriense 1
Ceratium contortum 3
Ceratium declinatum 1
Ceratium furca 21
Ceratium fusus 54
Ceratium macroceros v. gallicum 1
Ceratium hircus 86
Ceratium inflatum 1
Ceratium lineatum 1
Ceratium declinatum f. normale 2
Ceratium tripos v. ponticum 12
Ceratium sp. 1
Ceratium vultus v. sumatranum 1
Ceratium teres 3
Ceratium trichoceros 60
Ceratium tripos 76
Characium-like sp. 1
Family ..... Gonyaulacaceae
Gonyaulax sp. 1 1
Gonyaulax sp. 2
Gonyaulax diegensis 2
Phalocrama cuneus 1
Phalacroma sp. 2
Family ..... Pyrocystaceae
Pyrocystaceae pseudonoctiluca f. biconica 1
Pyrocystaceae sp.1 69
Family ..... Pyrophacaceae
Pyrophacus sp. 1
Pyrophacus horologium 2
Order ...... Prorocentrales
Family..... Prorocentraceae
Prorocentrum compressum 4
Prorocentrum gracile 7
Prorocentrum micans 18
Prorocentrum pyriformis 1
Prorocentrum sp. 1 2
Prorocentrum sp. 1
Prorocentrum triestinum 1
Division ... Chrysophyta.
Class ...... Chrysophycae (golden-brown algae)
Dictyocha fibula 29
Dictyocha fibula f. rhombica 1
Dictyocha sp. 1
Order ...... Chrysomonadales

Family ochromonadaceae
Dinobryon sertularia 8
Dinobryon sp. 3
Class Haptophyceae
Haptophyceae (haptophyte flagellate) 1
Division Xanthophyta
Class Xanthophyceae (yellow-green algae)
Xanthophyceae (yellow green falgellate) 2
Order Tribonemales
Family Tribonemataceae
Tribonema affine 2
Tribonema sp. 1
Division Bacillariophyta (diatoms)
Class Bacillariophyceae
Order Pennales
Suborder Araphidineae
Family Diatomaceae
Asterionella formosa 2
Asterionella japonica 5
Ctenophora pulchella 1
Delphineis livingstonii 2
Delphineis surirella 17
Dimerogramma marina 7
Dimerogramma minor 12
Falcual hyalina 39
Falcual media 1
Fragilaria capucina 3
Fragilaria construens 1
Fragilaria crotonensis 1
Fragilaria sp. 3
Fragilaria pinnata 2
Grammatophoa angulosa 1
Grammatophora oceanica v. macilenta 4
Grammatophora marina 41
Grammatophora oceanica 3
Grammatophora sp. 1
Licmophora abbreviata 5
Licmophora sp. 1
Neodelphineis pelagica 2
Opephora martyi 20
Opephora pacifica 6
Opephora schwartzii 30
Opephora sp. 3
Plagiogramma pulchellum 5
Plagiogramma pulchellum v. pygmaea 1
Plagiogramma sp. 1
Podcystis adriaticum 1
Rhabdonema adriaticum 93
Rhaphoneis amphiceros 1
Rhaphoneis liburnica 2
Rhaphoneis sp. 1
Striatella interrupta 3
Striatella unipunctata 46
Synedra aus 6
Synedra affinis 1
Synedra ulna v. amphirhyncus 3
Synedra crystallina 2
Synedra formosa 1
Synedra gaillonii 2

Synedra tabulata v. grandis 1
Synedra hennedyana 1
Synedra ulna v.oxyrhy. f.mediacontracta 1
Synedra ulna v. oxyrhynchus 11
Synedra acus v. radians 1
Synedra tabulata 24
Synedra toxoneides 1
Synedra ulna 18
Synedra undulata 2
Tabularia investiens I
Thalassionema nitzschioides 43
Thalassionema sp. 2
Thalassiothrix frauenfeldii 24
Thalassiothrix longissima 2
Thalassiothrix mediterranea 3
Thalassiothrix mediterranea v. pacifica 1
Family ..... Protoraphidaceae
Pseudohymantidium sp. 1
Suborder...Raphidineae
Family ..... Eunotiaceae
Eunotia alpina 4
Eunotia bidentula 1
Eunotia exigua 1
Eunotia lunaris 1
Eunotia monodon 2
Eunotia pectinalis 11
Eunotia praerupta 1
Eunotia sp. 4
Family ..... Achnanthaceae
Achnanthes brevipus 8
Achnanthes clevei 1
Achnanthes lanceolata v. dubla 1
Achnanthes exigua 2
Achnanthes haukiana 2
Achnanthes sp. 6
Anorthoneis excentrica 1
Cocconeis placentula v. euglypta 1
Cocconeis placentula I
Cocconeis scutellum 60
Cocconeis sp.
Family ..... Naviculaceae
Amphipleura pellucida 1
Amphiprora alata 3
Amphiprora gigantea 26
Amphiprora alata f. minor 1
Amphiprora pulchra 3
Amphiprora sulcata 2
Amphiprora sp. 1 1
Amphiprora sp. 1
Amphiprora gigantea v. sulcata 1
Amphora alata 1
Amphora angulosa 1
Amphora arcus 2
Amphora arenaria 1
Amphora cingulata 2
Amphora coffeaeformis 3
Amphora commutata 3
Amphora ocellata v. elongata 1
Amphora gigantea v. fusca 1
Amphora gigantea 1

Amphora holsatica 1
Amphora proteus v. maxima 1
Amphora mexicana 1
Amphora obtusa v. oceanica 1
Amphora obtusa 15
Amphora ocellata 3
Amphora ostrearia 1
Amphora ovalis 8
Amphora pediculus 2
Amphora proteus 9
Amphora obtusa v. rectangulata 1
Amphora sp. 1 2
Amphora sp. 2 3
Amphora sp. 3 1
Amphora sp. 4 1
Amphora sp. 9
Amphora sp. (small) 1
Amphora valida 1
Caloneis sp. r265 1
Caloneis acutiascula 1
Caloneis branderi 1
Caloneis latiascula 2
Caloneis libes 2
Caloneis maxima 1
Caloneis sp. 2
Caloneis westii 1
Capartogramma crucicula 2
Cymbella affinis 1
Cymbella aspera 1
Cymbella sp. 3
Diploneis adrena 1
Diploneis bombos 2
Diploneis crabro 4
Diploneis sp. 1
Diploneis ovalis v. oblongella. 1
Diploneis ovalis 16
Diploneis puella 1
Diploneis smithii 17
Frustulia rhomboides 1
Gomphonema angustatum 4
Gomphonema constrictum 1
Gomphonema gracile 1
Gyrosigma acuminatum 3
Gyrosigma attenuatum 1
Gyrosigma balticum 1
Gyrosigma simile 1
Gyrosigna sp. 6
Mastogloia angulata 14
Mastogloia apiculata 4
Mastoneis biformis 3
Mastogloia braunii 2
Mastogloia Cyclops 2
Mastogloia erythraea 3
Mastogloia hustedtii 3
Mastogloia lanceolata 1
Mastogloia macdonaldii 1
Mastogloia omissa 1
Mastogloia ovalis 1
Mastogloia portierana 1
Mastogloia rhombica 1

Mastogloia sp. 3
Mastogloia suboculata 1
Mastogloia varians 1
Navicula ambigua-like 1
Navicula cf. ammophila 3
Navicula bailyana 3
Navicula bioculata 1
Navicula clavata 6
Navicula granulata v. constricta 1
Navicula cryptocephala 3
Navicula directa 7
Navicula distans 1
Navicula irroratoides f. elliptica 1
Navicula forcipata 1
Navicula gracilis 1
Navicula gregaria 2
Navicula granulata 6
Navicula henneydi 1
Navicula irrorata 2
17
Navicula lyra
Navicula marina 1
Navicula monilifera 1
Navicula pinnata 1
Navicula pupula 1
Navicula scopularm 2
Navicula sp. 1 3
Navicula sp. 2 3
Navicula sp. 3 2
Navicula sp. 4 2
Navicula sp. 9
Navicula sp. (very small) 1
Navicula viridula 2
Navicula yarrensis v. americana 8
Navicula yarrensis 33
Navicula zanardiniana
Pinnularia gibba
Pinnularia sp.
Pinnularia viridis
Pleurosigma balticum
Pleurosigma delicatum
Pleurosigma elongatum 4
Pleurosigma formosum 11
Pleurosigma naviculaceum 1
Pleurosigma sp. 2 1
Pleurosigma speciosum 1
Pleurosigma sp. 4
Pleurosigma sp. 1 1
Pleurosigma sulcata 1
Stauroneis anceps 1
Stauroneis pachycephala 3
Stauroneis smithii 1
Stauroneis spicula 6
Trachyneis aspera 1
Tropidoneis lepidoptera 8
Tropidoneis sp. 1
Family ..... Epithemiaceae
Rhopalodia gibba 4
Rhopalodia gibberula 4
Family ..... Nitzschiaceae
Bacillaria paradoxa 23

Bacillaria paxillifer 20
Hantzschai sp. 2
Nitzschia acuminata 1
Nitzschia angularis 1
Nitzschia circumsuta 1
Nitzschia acicularis v. closterioides 8
Nitzschia clarissima 1
Nitzschia coarctata 1
Nitzschia constricta 2
Nitzschia closterium 14
Nitzschia delicatissima 1
Nitzschia gartlopii 1
Nitzschia sigma v. habirshawii 1
Nitzschia incurva 1
Nitzschia Insignis 3
Nitzschia jelinecki 1
Nitzschia lanceolata 3
Nitzschia longa 10
Nitzschia longissima 17
Nitzschia lorenziana 7
Nitzschia macilenta 1
Nitzschia maxima 2
Nitzschia obtusa 5
Nitzschia palea 2
Nitzschia panduriformis 4
Nitzschia paradoxa 1
Nitzschia punctata 3
Nitzschia pungens 3
Nitzschia longissima v. reversa 2
Nitzschia rigrida 1
Nitzschia lorenziana v. subtilis 1
Nitzschia scalaris 2
Nitzschia seriata 7
Nitzschia sigma 26
Nitzschia sigma v. sigmatella 1
Nitzschia sigmoidea 5
Nitzschia socialis 1
Nitzschia Sp. 1 1
Nitzschia sp. 2 1
Nitzschla sp. (arc shaped) 1
Nitzschia SP 15
Nitzschia tryb1ionella v. subsalina 1
Nitzschia triblionella v.salinarum 1
Nitzschia triblionella 10
Nitzschia longissima v. typica 1
Nitzschia valida 2
Pseudoeunotia doliolus 1
Pseudoeunotia sp. 1
Family ..... Surirellaceae
Campylodiscus clypeus 5
Campylodiscus echeineis 4
Campylodiscus eximius 2
Campylodiscus imperialis 2
Campylodiscus limbatus 7
Campylodiscus samoensis 1
Campylodiscus sp. 1
Surirella sp. r265 1
Surirella fastuosa v. cuneata 1
Surirella fastuosa 1
Surirella gemma 6

Surixella robusta f. minor 1
Surirella tenera v. nervosa 1
Sur1rella ovata 3
Surirella ovalis 2
Surirella fastuosa v. recedens 1
Surirella robusta 3
Surirelia sp. 1 1
Surirella sp. 1
Surirella tenera 3
Order ...... Centrales
Suborder ... Coscinodiscineae
Family ...... Thalassiosiraceae
Aulacosira granulata v. angutissima 1
Aulacosira granulata 8
C clotella meneghiniana 38
6Y
C6yclotella sp. 1 3
Cyclotella sp. 2 1
Cyclotella sp. 7
Cyclotella sp. (small) 97'
Cyclotella striata 88
Cyclotella stylorum 8
Lauderia borealis 1
Lauderia compressa 1
Skeletonema costatum 19
Thalassiosira decipiens 9
Thalassiosira eccentrica 26
Thalassiosira gracilis 3
Thalassiosira lineatus 3
Thalassiosira nannolineata 4
Thalassiosira oestrupli 40
Thalassiosira sp. 1 1
Thalassiosira sp. 2 1
Thalassiosira sp. 13
Thalassiosira, sp. (small) 4
Family......Melosiraceae
Corethron hystrix 4
Corethron pelagicum 1
,Hyalodiscus radiatus 3
Leptocylindrus danicus 26
Leptocylindrus-like 1.
Melosira (aulacosira) 6ranulata 1
.Melosira ambigua 1
Melosira borresi I
8Melosira dubia 6
8Melosi-ra ranulata 4
Melosira luercrensii 1
Melosira moniliformis 2
08Melos0ira undulata v, morani4l 61
Melos4i8ra undulata v. nozman4ii 61
Melos0i0ra nummulo0ides 4
08Melos4ira sp. 3
Melos4i4ra undulata 2
04Melosi4ra var4ians 16
44Pa8ralia sulca0ta v. b0iseriata 2
Pa8ralia sulcata f. coronata 4
Pa4ral6ia sulcata 46
Podos4iza stelli16er 3
Stephanop16yxis turris 5
Family ..... Hemidiscaceae
Actinocyclus crassus 01

Actinocyclus curvatulus 1
Actinocyclus ehrenbergii 58
Actinocyclus ehrenbergii v. ralfsii 5
Actinocyclus ralfsii 2
Actinocyclus ralfsii v. sparsus 1
Actinocyclus sp. 4
Actinocyclus tennuissimus 1
Actinocyclus ehrenbergii v. tenella 2
Hemidiscus cuneiformis
Actinoptychus senarius 2
Actinoptychus undulatus 30
Family ..... Asterolampraceae
Asteromphalus flabellatus 3
Asteromphalus heptactis 1
Family ..... Eupodiscaceae
Auliscus caelatus 1
Triceratium favus 2
Triceratium sculptum 1
Triceratium spinosum 1
Triceratium sp. 1
Family ..... Chaetoceraceae
Bacteriastrum delicatulum 2
Bacteriastrum elongatum 2
Bacteriastrum hyalinum 34
Bacterlastrum hyalinum v. princeps 1
Bacteriastrum varians 15
Chaetoceros affinis 15
Chaetoceros atlanticus 1
Chaetoceros didymus v. atlanticus 1
Chaetoceros brevis 75 Chaetoceros brevis 75
Chaetoceros convolutus 1
Chaetoceros coarctatus 42
Chaetoceros compressus 7
Chaetoceros constrictus 5
Chaetoceros costatum 4
Chaetoceros crinitus 1
Chaetoceros curvisetus 8
Chaetoceros danicus 2
Chaetoceros debile 3
Chaetoceros decipiens 97
Chaetoceros densus 20
Chaetoceros didymus 90
Chaetoceros diversus 1
Chaetoceros eibonii 10
Chaetoceros filiformis 1
Chaetoceros furcellatus 3
Chaetoceros qracilis 10
Chaetoceros laciniosus 38
Chaetoceros lauderi 24
Chaetoceros lorenzianus 31
Chaetoceros mediterranea 1
Chaetoceros messanensis 16
Chaetoceros pelagicus 10
Chaetoceros pendulus 2
Chaetoceros didymus v. protuberans 32
Chaetoceros pseudocurvisetus 6
Chaetoceros radicans 1
Chaetoceros socialis 77
Chaetoceros sp. 1

Chaetoceros wigami 1
Cymatosira belgica 2
Cymatosira lorenziana 19
Family ..... Lithodesmriaceae
Ditylum brightwelli 2
Lithodesmium undulatum 3
Streptotheca indica 1
Family ..... Rhizosoleniaceae
Guinardia flaccida 11
Rhizosolenia alata 23
Rhizosolenia calcaravis 9
Rhizosolenia delicatula 5
Rhizosolenia fragilissima 6
Rhizosolenia alata f. gracillima 2
Rhizosolenia hebetata
Rhizosolenia imbricata 13
Rhizosolenia alata f. indica 2
Rhizosolenia alata v. inervis 1
Rhizosolenia styliformis v. longispina 1
Rhizosolenia robusta 2
Rhizosolenia hebetata v. semispina 2
Rhizosolenia setigera 8
Rhizosolenia imbricata v. shrubsolei 2
Rhizosolenia stolterfothii 54
Rhizosolenia styliformis 8
Family ..... Coscinodiscaceae
Coscinodiscus apiculatus v. ambigua 1
Coscinodiscus apiculatus 4
Coscinodiscus argus 1
Coscinodiscus asteromphalus 4
Coscinodiscus centralis 154
Coscinodiscus concinnus 1
Coscinodiscus curvatulus 4
Coscinodiscus divisus 1
Coscinodiscus granii 123
Coscinodiscus janischii 1
Coscinodiscus marginatus 3
Coscinodiscus obscurus 3
Coscinodiscus oculus-iridis 8
Coscinodiscus operculatus 2
Coscinodiscus perforatus v. pavillardii 2
Coscinodiscus perforatus 12
Coscinodiscus radiatus 5
Coscinodiscus sp. 4
Psammodiscus nitidus 3
Stellarima microtrias 1
Suborder ... Biddulphiineae
Family ..... Biddulphiaceae
Anaulus sp. 1
Attheya decora 1
Biddulphia laevis 1
Biddulphia mobiliensis 5
Biddulphia regia 1
Biddulphia sinensis 5 Ethmodiscus sp. 1
Eucampia zoodiacus 2
Eunatogramma laevis 1
Eunatogramma weissei 2
Hemiaulus hauckii 19
Hemiaulus membranacea 1

Hemiaulus sinensis
Hydrosera whampoensis
Terpsinoe americana
Terpsinoe intermedia
Division ... Chlorophyta
Class ...... Chlorophyceae (green algae)
Order ...... Chlorococcales
Family ..... Hydrodictyaceae
Pediastrum biradiatum 3
Pediastrum simplex v. duodenarium 2
Pediastrum simplex 5
Family ..... Scenedesmaceae
Scenedesmus quadricauda 1
Order ...... Ulotrichales
Family ..... Microsporaceae
Microspora sp. 1 1
Microspora sp. 2 1
Mi crospora sp. 1.
Order ...... Volvocales
Unidentified green flagellates 1
Family ..... Volvocaceae
Volvox aureus 1
Order ...... Zyqnemales
Family ..... besmediaceae
Closterium sp. 1 1
Closterium sp. 2 1
Microsterias sp. 1
Staurastrum notatum 1
Staurastrum paradoxum 2
Family ..... Zygnemaceae
Mougeotia sp. 1 (narrow trichomes) 2
Mougeotia sp. 2 (wide trichomes) 1
Mougeotia sp. 3 1
Mougeotia sp. 4 2
Mougeotia sp. 3

Systematics unknown or unassigned
Dissodnium sp. 1
Unidentified flagellates 20

Systematic review

Offshore (gulf) stations, day, surface

No. of occurrences
Division ... Cyanophyta
Class ...... Cyanophyceae (blue-green algae*or cyanobacteria)
Order ...... Chroococcales
Family ..... Chroococcaceae
Eucapsis Sp. 2
Order ...... Nostocales
Family ..... Oscillatoriaceae
Microcoleus lyngbyaceus 7
oscillatoria membranacea 1.
Schizothrix sp. 1
Trichodesmium erythreaum 7
Division ... Dinophyta
Class ...... Dinophyceae (dinoflagellates)
Order ...... Peridiniales
Family ..... Peridiniaceae
Peridinium conicum 6
Peridinium elegans 1
Peridinium nipponicum 1
Pe.ridinium oblongum 13
Perldinium sp. 2
Family ..... Protoperidiniaceae
Diplopsalis lenticula 6
order ...... Dinophysiales
Family ..... Dinophysiaceae,
Cladop_yxis brachiolata 2
Dinophysis caudata 7
Ornithoceros magnificus 2
Oxytoxum Sp. 2
Order ...... Gonyaulacales
Family ..... Ceratiaceae
Ceratium furca 13
Ceratium fusus 9
..Ceratium hircus 5
Ceratium teres 3
CeratiLun trichoceros 12
Ceratium tripos 5
Ceratium vultar 1
Family ..... Gonyaulacaceae
Gonyaulax monilata 1
Family ..... Pyrocystaceae
Noctiluca marina 1
Family ..... Pyrophacaceae
Pyrophacus horologium 1
Family ..... Ceratocoryaceae
Ceratocorys h<)rrida 4
Order ...... Prorocentrales
Family ..... Prorocentraceae
Prorocentrum gracile I
Prorocentrum micans 2
Prorocentrum minimum 1
Division ... Bacillariophyta (diatoms)

Class ...... Bacillariophyceae
Order ...... Pennales
Suborder ... Araphidineae
Family ..... Diatomaceae
Asterionella sp. 1
Asterionella japonica 2
Delphineis livingstonii 1
Delphineis surirella 2
Dimerogramma marina 1
Plagiogramma-like sp. 2
Plagiogramma sp. 1
Rhabdonema adriaticum 5
Striatella unipunctata 5
Thalassionema nitzschioides 6
Thalassiothrix frauenfeldii 13
Thalassiothrix longissima 2
Thalassiothrix mediterranea 2
Thalassiothrix mediterranea v. pacifica 3
Suborder ... Raphidineae
Family....Naviculaceae
Amphiprora gigantea 1
Amphora obtusa 1
Gyrosigma macrum 1
Haslea sp. 1
Navicula granulata 1
Navicula sp. (needle type) 2
Pleurosigma angulatum 5
Family ..... Nitzschiaceae
Bacillaria paxillifer 1
Nitzschia closterium 3
Nitzschia longissima 3
Nitzschia pungens 3
Nitzschia seriata 1
Nitzschia sigmoidea 1
Family ..... Surirellaceae
Campylodiscus echeineis 1
Order ...... Centrales
Suborder ... Coscinodiscineae
Family ..... Thalassiosiraceae
Cyclotella striata 1
Skeletonema costatum 11
Thalassiosira eccentrica 6
Thalassiosira oestrupii 4
Family.......Melosiraceae
Leptocylindrus danqicus 2
Paralia sulcata 1
Podosira stelliger 5
Stephanopyxis palmeriana 6
Stephanopyxis turris 3
Family ..... Hemidiscaceae
Actinocyclus ehrenbergii 3
Azpeitia nodulifer 1
Hemidiscus cuneiformis 3
hemidiscus sp. 4
Family ..... Heliopeltaceae
Actinoptychus senarius 2
Family ..... Eupodiscaceae
Aulacodiscus argus 3
Auliscus sculptus 1

Eupodiscus radiatus 2
Family ..... Chaetoceraceae
Bacteriastrum varians 16
Chaetoceros affinis 3
Chaetoceros atlanticus 1
Chaetoceros brevis 10
Chaetoceros coarctatus 2
Chaetoceros curvisetus 2
Chaetoceros decipiens 8
Chaetoceros densus 1
Chaetoceros didymus 4
Chaetoceros diversus 8
Chaetoceros eibonii 1
Chaetoceros lauderi 1
Chaetoceros lorenzianus 1
Chaetoceros messanensis 1
Chaetoceros peruvianus 6
Chaetoceros pseudocurvisetus 1
Chaetoceros teres 1
Cymatosira belgica 5
Cymatosira lorenziana 2
Family ..... Lithodesmiacae
Bellorochea malleus 1
Dqitylum brightwelli 5
Lithodesmium undulatum 3
Family ..... Rhizosoleniaceae
Corethron cryophyllum 1
Dactyliosolen sp. 1
Detonula sp. 1
Guinardia flaccida 16 Rhizosolenia alata 15
Rhizosolenia calcaqravis 6
Rhizosolenia imbricata 18
Rhizosolenia alata f. indica 1
Rhizosolenia robusta 15
Rhizosolenia setigera 11
Rhizosolenia stolterfothii 16
Rhizosolenia styliformis 6
Rhizosolenia castracanii 9
Family ..... Coscinodiscaceae
Coscinodiscus centralis 9
Coscinodiscus concinnus 3
Coscinodiscus granii 5
Coscinodiscus jonesianus 3
Coscinodiscus operculatus 1
coscinodiscus radiatus 3
Stellarima microtrias 1
Suborder ... Biddulphiineae
Family ..... Biddulphiaceae
Biddulphia mobilensis 4
Biddulphia rhombus 1
Biddulphia sinensis 10
Biddulphia sinensis-like 1
Biddulphia titian 1
Climacodium frauenfeldianum 8
Ditylum sp. 1
eucampia cornuta 1
Eucampia zoodiacus 11
Hemiaulus membranacea 5
Hemiaulus sinensis 7

Streptotheca thamensis

hVVV) W-1 bib
diversity taken monthly from September, 1985 through
August, 1986.

500000

7-N
400000 -

Q
CD
Q 15-N
300000 -
x
22-N
CI)

25-N
LU 200000-

31-N
z

34-N
100000-

36E-N

38-N

LO U) U) LO to CD (D co co co (0 CD
00 OD 00 00 OD CD OD 00 00 co
cq LO Go

DATE

CHUCIAWHA)UHLE bAY ALGAE: 64 MICRO-M

6o-
13 3-NSPP

7-NSPP
50- 0
A.
V. 11 -NSPP

15-NSPP
40-
Cl)

LLI let
'o,
--w- 19-NSP

30- 22-NSPP
cn
LU
25-NSPP
LU 2o-

31 -NSPP

34-NSP
10-

---0--- 36E-NSPP

o 38-NSPP
ul) Ln Ln LO co co ro 11 CD co co
co Co. co co co co OD CD co co
(D C@ N co Ln w rz co

DATE

CHOCATWHATCHLF- bAY ALUAt: b4 MICHO-M

4-
3-SHAN.DIV.

7-SHAN.Div.

11 -SHAN.DIV.

15-SHAN.DIV.
3-

LLJ 19-SHAN.Div.
b
>
ES
13 22-SHAN.DIV.
z
0
z
25-SHAN.DIV.
z
2-

31 -SHAN.Dlv.

34-SHAN.DIV.

---0--- 36E-SHAN.DIV.

38-SHAN.DIV.
U) LO U*) Ul) co co co w w flo co co
00 co co co co co co co co co
a N co LO co r- co

DATE

levels noted in winter months. Most of the other bay stations had relatively low

species richness levels during most times of the year. With the exception of

January, 1986 (the time of high numbers and high dominance), the species

diversity was also highest at -these two western stations. Such diversity indices

were uniformly high at all other times of the year. In this way, eutrophicated

conditions were characterized by high numbers of phytoplankton, high

phytoplankton species richness and high diversity.

The dominant algal species in the Choctawhatchee Bay system over the

period of study were run against the various important water quality factors as a
distribution analysis by increments. The number of occurrences of specific

ranges of important physical/chemical factors are shown graphically (Figure 8)

along with the occurrences of dominant phytoplankton species along such

gradients. - Salinity levels in the bay were scattered across a relatively wide

range with the highest frequencies of occurrence between 8 and 24 ppt. The
phytoplankton species were located along gradients of salinity. For instance,
Chaetoceros brevis was located along the mid-range'of salinity whereas C.

didymus was an indicator of higher salinities. Other species, such as

Skeletonerria costatum, were ranged along the lower levels of salinity. Most of

the phytoplankon species showed specific ranges of salinity tolerance within

varying ranges.

Dissolved oxygen (Figure 8) was relatively high at the surface of the bay

throughout the year with levels remaining generally higher than .5. mg1l. Most of

the phytoplankton were found at levels between 6.0 and 9.0 mg/l. The relative

differences probably reflected seasonal changes in temperature and D. 0.

rather than any species-specific changes along D. 0. gradients.

kkitiom, wikkiiwab, biiu Giolukcopkiyn a. ine numerically
dominant phytoplankton species (16) are tested as possible
indicators of water quality phenomena in the Choctawhatchee
Bay system from September, 1985 through August, 1986.

30-

Cn
LU

z
LU 20-

10-

CD 0 OD C\1
C14 C\j CY)

SALINITY: CLASS MIDPOINTS

28-
LU 24
Chaetoceros brevis
z 20
El Chaetoceros coarctatus
LLI 16-
El Chaetoceros decipiens
El Chaetoceros didymus
12
Chaetoceros socialis
8 -

4
113
NEON I
0 T
C\l 0 Co C\j (D
C\j C\j CV)
SALINITY: CLASS MIDPOINTS

40-

LU
C) 30- Coscinodiscus centralis
z El Falcula hyalina
LU El Rhizosolenia stolterfothii
(t 20 - Cocconeis scutellum
cc Cyclotella striata
M 10- Navicula cf. ammophila

0 (D
cli 00 C\j
Cl)
SALINITY: CLkSS MIDTPOINTS

20-

LU 16-
Pyrocystis sp. 1
z
LU 12- Rhozosolenia delicatula
1= ED Skeletonema costatum
8- Thalassiosira oestakupii
Thalassionema nitzschioides

4
0,
Co Co Cq
17 C\j C\l C9 CY)
SALINITY: CLASS MIDPOINTS

CHOCTAWHATCHEE BAY 64 MICRO-M SAMPLES

50-

40-

cl)
LLI 30-
U
z

20-
U

10-

0.-
tn Ln Ln U@ Lq U.) Lo U-) U) Ln
U) U)
N cr) ui (6 C6 0;

DISSOLVED OXYGEN: CLASS MIDPOINTS

uu -
LU 40-
U Chaetoceros brevis
z 30
LU El Chaetoceros coarctatus
cc EN Chaetoceros decipiens
2o- El Chaetoceros didymus
El Chaetoceros socialis
C) 10-
L)
0
Lo Ln
IQ Ui Ln U) Lo in Ul) Lo Lo
rn
DI��'OLVED OXYGEN: 6LASS' MIDPOINTS

50-
U)
LLJ 40-
Cocconeis scutellum
z Coscinodiscus centralis
LLJ 30-
Cyclotella striata
Falcula hyalina
20-
Navicula cf. ammophila
Pyrocystis sp. 1
10

0
0
Lq Lq Lq Li U@ Lq Lq U@ Ui Ui Lq Li
Dld'@OLVED O'X Y G'E'N: &LAS9 'MIDPOINTS.

2o-

LU
Rhizosolenia delicatula
z
LU El Rhizosolenia stolterfothii
10- 0 Skeletonema costatum
El Thalassiosira oestrupii
El Thalassionema nitzschioides
0
0
0
Lf) ti) L,) Lr) U) Lr) V) U) U) L0 L0 Lr)
C@ oi .4 vi (6 C6 oi C;
DISSOLVED OXYGEN: CLASS MIDPOINTS

I u
cf)
LU 8-
z Chaetoceros brevis
LU 6- El Chaetoceros coarctatus
IN Chaetoceros decipiens
4 El Chaetoceros didymus
El Chaetoceros socialis
2

U) Lr) Lo Lo Lf) Lo Lo Lo Ln
DISSOL'Vn %O'k Y G F- N: 'CLASS MIDPOINTS

15-
cl)
LU

Coscinodiscus centralis
z 10- Falcula hyalina
LU
El Rhizosolenia stolterfothii
Cocconeis scutelium
5 Cyclotella striata
Navicula ammophila

0
Lo to U) Lo Lo U) U) U) Lo Lq Lq
0
EFISS(YLVEt ORYGtN: CLOS MIDP61NTS

6-
cl) 5-
uj
4- Pyrocystis sp. 1
z
LLJ Rhizosolenia delicatula
3- E3 Skeletonema costatum
Thalassiosira oestrupii
2-
El Thalassionema nitzschioides

L,) Lf) Lc) Lf) Lr) Lc) Lc) Lo Lo Ln
c; c@ C6 4 L6 C6 r-@ 06 a; c;
DISSOLVED OXYGEN: CLASS MIDPOINTS

GHUL,'kAVVk-lA'kt,htt 6AY b4 lVllt.;H0-tVl SAIVIVILtS

30-

20-

LLJ

z
LU

L)
L)
0 10-

0
Ul) r- 0) cv) P, 0) c) U-) co
ci
Q 0 0 c@ c@ 04 c\l c@

SECCHI DEPTHS: CLASS MIDPOINTS

30-
Cf)
LLI

20- Chaetoceros brevis
LLJ Chaetoceros coarctatus
El Chaetoceros deciplens
Chaetoceros didymus
10-
El Chaetoceros socialis
0 L.,in., Lb .0 'k
o4
17 Ci LQ O@ Ci Iq 0! Ci U@
0 C@ 0 C5 a Cm
RECCHI DEPTH: CLARS MIDPOINTS A

15-
U)
LU

z 10 Rhizosolenia delicatula
LU Rhizosolenia stolterfothii
W Skeletonbma costatum
Thalassiosira oestrupii
5 El Thalassionema nitzschioides

nn
0
q Lq cl, LQ Ci LQ CR
Q 0 0 C) 0 N N C\l C\j C\j
SECCHI DEPTHS: CLASS MIDPOINTS A

30-
Cf)
LU
0 N cocconeis scutellum
z 20- 9 Coscinodiscus centralis
LU El Cyclotella striata
cc Falcula hyalina
10- Navicula cf. ammophila
U
U
d
Pyrocystis sp. 1

0
j:
o4- m E3 I 3m3 L.
Ci LQ a! V) Cf) W) Co
C> 0 C) C3 C@ C@ C-j C@ C@
RECCHI DEPTH: MIDPOINTS A

CHOCTAWHA'i GHEL BAY 64 MICRO-M SAMPL5S

200-

U)
LU

z
LU 100-

0
cy) U) cy) cy) L0 cy)
6 6

PHOSPHATE: CLASS MIDPOINTS

1()U
w 80-
C)
z Chaetoceros brevis
LLI 60- El Chaetoceros coarctatus
El Chaetoceros decipiens
40 Chaetoceros didymus
Chaetoceros socialis
20

0-
N
C@ @2
PH6SPHATE: CLASS MIDPOIRT$ A

200-
U)
w

Cocconeis scutellum
z Coscinodiscus centralis
LU E3 Cyclotella striata
X 100-
Falcula hyalina
El Navicula cf. ammophila
Pyrocystis sp. 1

0
0-
-
Cl) CY) CO) Lo N G) C\J
C) 0
C@ C@
-4 6 6
PHOSPHATE: CLASS MIDPOINTS A

60-
Cn
LLJ 50-

z 40- Rhizosolenia delicatula
w Rhizosolenia stolterfothii
cc 30- z E3 Skeletonema costatum
Thalassiosira oes'trupii
20- = El Thalassionema nitzschioides
L)
10-

0
co Lo CO U') N N
C@ 7 7
n F 5' cl
PHOSPHATE: CLASS MIDPOINTTS c) A

CHOCTAWHATCHEE BAY 64 MICRO-M SAMPLES

80-

60-

(n
LU

z
LU 40-

cc
D

20-

0
Lo Lo Lo Lo U) Lo Lo Ln Lo Ln cy)
It fl- 0 cy) co 0) c\j Lo 00 C5
q c@ IR c\j C\! c@ 11
0 0 C3 0 0 A

NITRATE: CLASS MIDPOINTS

bo -

U.1
0 40-
z Chaetoceros brevis
uj 30- Chaetoceros coarctatus
Chaetoceros decipiens
20- Chaetoceros didymus
El Chaetoceros socialis
L) 10-
C) F-P.1
0 m-n
0 -Mill m..". .1 m. mail
Ln Lo Ln Lo Lo U) Ln Lo U) cl
P, 0 Cl) C\j U) 00
C@ NI
TRATE: CLASS MIDPOINf@
0 0 0 0 A

80-

LLI
U 60- Cocconeis scutellum
z
Ill El Coscinodiscus centralis
40- Cyclotella striata
Falcula hyalina
El Navicula cf. ammophila
20 Pyrocystis sp. 1
L)
0 A m ER_ - RL Au lh, m
U) In U') in 0 to w U') U) U*) CY)
C0 04 LI) co
'D 0' C@
NITRATE: CLASS MIDPOINf@
0 A

30-
W
LLJ

z 20- Rhizosolenia delicatula
LU Rhizosolenia stolterfothii
El Skeletonema costatum
Thalassiosira oestrupii
10-
Thalassionema nitzschioides
L)
U
r-, n @k n F A
ol@ 4-2--1-1 g Fh. ffin]
U) Lo Ln Lo W Lo Lo Ln Lo Co
rl 0 0 w Cq U') Co
C! 17 17 C\! C\! C@
NITRATE: CLKSS MIDPOINTS 0 A

CHUU'k AWHA'k GHEL bAY b4 #Vll(;HU-lVfSAiVl-PLtS

80-

60-

cl)
w
L)
z
w 40-

M
L)
L)
0

20-

0-
co q* C) co c\j co ..t 0 co c\l CD
C) c\j Lo N 00 C3 cq cl) Lo
c@ CR c@ CR c@ q 7
0 0 C) 0 0 0 c@
A

AMMONIA: CLASS MIDPOINTS

bu
W
w 40-
z Chaetoceros brevis
LU 30 - Chaetoceros coarctatus
ix El Chaetoceros decipiens
cc 20 El Chaetoceros didymus
D Chaetoceros socialis
10
I ULU I
PM
0 rm
00 (D N 00 0 co C\l (D
0 Cq U) r- co 0 C\l Cl) U)
0 0 in - 1@ C;
C; c; AMMONIA: CLASS MIDPOINfS o 0 11
A

80-
Cf)
LLJ
60- Cocconeis scutellum
z El Coscinodiscus centralis
LLI
Cyclotella striata
cc 4o-
cc Falcula hyalina
El Navicula cf. ammophila
20 Pyrocystis sp. 1

min
0- Am. m'. - Am 0
00 C@ Co C\l 00 'T 0 W C\j (D
(D cli Ln I-- Co 0 C\l Cl) Lo
C@ C@ 0 0 0 0 - . - - - 6
0 0 C; AhAMON0k! cl-Ass mibPOINt.9 11
A

25-

Cl)
uj 20-
z 15- Rhizosolenia delicatula
w Rhizosolenia stolterfothii
m Skeletonema costatum
cc 10 Thalassiosira oestrupii
M El Thalassionema nitzschioides
0 5-

0 M 13. n. w n. n
Co w Co 0 Cq
0 cm U) Co C) N Co to
C@ C@ C! C@ C@ C@ C;
0 0 0 11
AIMMONFA: CLASS MfDPOINTS A

UhUL,lAVVrlAlUn)=k= OA@ 014 gV11146,riV-11VI %->AIVIeLk=%*-i

40-

30-

U)
LLJ

z
ui 20-
cc
cc
M

10-

Ui U@ LQ LQ U) Lo Ln An Lo Ln 0
c\l r@ N r@ C\i r-@ c@ r-@ c@ r-: Lo
04 cli cy) ce) 11
A

CHLOROPHYLL A: CLASS MIDPOINTS

U) 30-

C)
z 20- Chaetoceros brevis
LLJ El Chaetoceros coarctatus
El Chaetoceros decipiens
Chaetoceros didymus
M 10-
Chaetoceros socialis
C)

0
U@ U) Ln Lr)
LQ U@ Lq Iq Lq Lo
0j 04 rl- C\j fl. C\j C\i 11
-CHLOROPHYLL A: _CLASS_ MIDPOINTS A

W 40-
LLJ 35-
30- Cocconeis scutellum
z
LU 25 Coscinodiscus centralis
Cyclotella striata
2o- Falcula hyalina
-:
15 Navicula cf. ammophila
Pyrocystis sp. 1
10-

5-
7h I
0 Lq ./
U@ Lq LQ LQ L0 U) U@ U) U@ Ln
Cq rl- Cm rl: C@ rl- C@ 1- 11
-CHLOROPHYLL A:-CLASS MIDPJOINTS 'q Nt A

20-
W
Lli
0 15-
z Rhizosolenia delicatula
LLJ Rhizosolenia stolterfothii
10- Skeletonema costatum
Thalassiosira oestrupii
El Thalassionema nitzschiold e*s
5-

R.. n
n.
n gm I
0-
Lq LQ to Lo Lo
LQ Lq Ui Lq U@ U)
cli r@ Cu 1@_ Cu rl: 6 r-: 11
CHLOROPHYLLA: CLASS MIDPOINTS A

Secchi depth distributions (Figure 8) were ranged around 1.5 m. The
species Pyrocysistis sp. 1 was located in high numbers at relatively low levels of
light penetration. Most of the other species were dominant at levels of relatively

high light penetration according to the Secchi readings (usually > 1.5 m). The

phosphate distributions were based on filtered samples; most such readings

were very low so that the data, as presented, may not be representative of the

response of phytoplankton to orthophosphate levels. The species Chaetoceros

brevis may be an indicator of high phosphate levels. The data will be run with

the unfiltered orthophosphate samples to verify this possibility. For now, these

findings remain preliminary. Most of the species of phytoplankton were found at

low levels of orthophosphate.

The nitrate distribution in the bay in terms of occurrence over the year-

long study (Figure 8) was weighted around the low end of the spectrum. Once
again, Chaetosceros brevis occurred at relatively high levels of nitrate which

could be establish this species as an indicator of high dissolved.nutrients. Other

species such as Thalassiosira oestrupii and Rhizosolenia stofterfothii were also

found in relatively high numbers at high concentrations of nitrate.Other

phytoplankton species were clustered at the low end of the nutrient spectrum.

Ammonia was also found to occur most frequently at the low end of the

concentration spectrum. Species such as Chaetoceros didymus, C. socialis,

and Rhizosolenia stolterfothii were indicators of high ammonia levels. Such

species were also found at low concentrations of ammonia which means that

they cannot be used as exclusive indica tors of high ammonia levels. Indicators

of chlorophyll a concentrations included most of the Chaetoceros species and i,
Coscinodiscus centralis, and Pyrocystis sp. 1.

In most instances, the various phytoplankton species were found along

relatively broad ranges of the various water quality distributions. This precludes

the use of any single indicator species as the sole representative of a particular
habitat condition. However, when used in conjunction with the various
community parameters, the phytoplankton as a group were higly indicative of
various water quality conditions with particular emphasis on salinity and the

nutrient distributions at culturally eutrophicated stations.

V. REFERENCES

Abbot, Markt, & Company. 1960. Supporting data on Choctawhatchee Basin.
Unpublished report.

Alabama Water Improvement Commission. 1976. Choctawhatchee River Basin:
water quality management plan. Unpublished report.

Edmondson, W. T. 1972. Nutrients and phytoplankton Lake Washington,pp.
172-193. In: Nutrients and eutrophication (G. Likens, Ed.) Amer. Soc. Limnol.
Oceanog. Spec. Symp. No. 1.

Florida Department of Environmental Regulation. 1980. Water quality inventory
for the state of Florida:1 980.

Florida Department of Environmental Regulation. 1986. 1986 Florida Water
Quality Assessment 305(b) technical report.

Federal Power Commission. 1966. Escambia-Choctawhatchee river basins
area. Unpublished report.

Geissler, U. and R. Jahn. 1986. Infraspecific taxa of diatoms as indicators of
water quality? M. Ricard, Ed.. Proceedings of 8th Diatom-Symposium.
Ottokoeltz, Konigstein, Germany. pp. 766-771.

Livingston, R. J. 1984. Trophic response of fishes to habitat variability in coastal
seagrass systems. Ecology 65: 1258-1275.

Livingston, R.J. 1984. The ecology of the Apalachicola Bay system: an estuarine
profile. U. S. Fish Wildl. Serv. FWS/OBS 82/05.148 pp.

Livingston, R. J. 1985. Field verification of bioassay results at toxic waste sites in
three southeastern drainage systems. Unpublished report.

Livingston, R.J. 1986a. The Choctawhatchee River-Bay system. Unpublished
report.
r

Livingston, R. J. 1986b. Preliminary report. Analysis of field data concerning Old
Pass Lagoon (Choctawhatchee Bay, Florida: September, 1985-February,
1986). Unpublished report.

Livingston, R. J. 1987. Distribution of toxic agents and biological response of
infaunal macroinvertebrates in the Choctawhatchee Bay system. Unpublished
report for the Northwest Florida Water Management District and the Office of
Coastal Management, Florida Department of Environmental Regulation.

Livingston, R. J., J. Jimeian, F. Jordan, and S. E. McGlynn. 1988. The ecology of
the Choctawhatchee River system. Unpublished report for the Northwest Florida
Water Management District.

Maestrini, S. Y., D. J. Bonin, and M. R. Droop. 1984. Phytoplankton as indicators
of sea water quality: Bioassay approaches and protocols. pp. 71-132. In:
Shubert, L. E. Algae as Ecological Indicators. Academic Press. New York, New
York.

Marshall, H. G. 1982. Meso-scale distribution patterns for diatoms over the
northeastern continental shelf of the United States. D. Mann,.Ed. Proceedings
of 7th Diatom-Symposium. Ottokoeltz, Konigstein,.Germany. pp. 393-400.

Northwest-Florida Water Management District. 1980. Initial investigation tow ard
the development of a management program for Choctawhatchee Bay, Florida.
Unpublished report.

Patrick, R. 1986. Diatoms as indicators of changes in water quality. M. Ricard,
Ed. Proceedings of 8th Diatom-Symposium. Ottokoeltz, Konigstein, Germany.
pp. 759-765.

Potts, M. 1980. Blue-green algae (Cyanophyta) in marine coastal environments
of the Sinae Peninsula; distribution, zonation, stratification and taxonomic
diversity. Phycologia 19, 60-73.

Prasad, A. K. S. K. and R. J. Livingston. 1987. An atlas of diatoms and other
algal forms from selected drainage areas in central and north Florida;
Unpublished report for the Florida Department of Environmental Regulation).

Premila, V. E. and M. Umamaheswara Rao. 1977. Distribution and seasonal
abundance of Oscillatoria nigroviridis Thwaites ex. Gomant in the waters of
Visakhapatnam Harbour. Ind. J. Mar. Sci. 3, 79-91.

Reddy, P. M. and V. Venkateswarlu. 1986. Ecology of algae in the paper mill
effluents and their impact on the river Tungabhadra. J. Environ. Biol. 7, 215-
223.

Schoeman, F. R. and E. Y. Haworth. 1986. Diatoms as indicators of pollution.
M. Ricard, Ed. Proceedings of 8th Diatom-Symposium. Ottokoeltz, Konigstein,
Germany. pp. 757-759.

Shubert, L. E. 1984. Algae as Ecological Indicators. Academic Press. New York,
New York.

Squires, L. E. and N. A. Sinnu. 1984. Seasonal changes in the diatom flora in
the estuary of the Damour River, Lebanon. D. Mann, Ed. Proceedings of 7th
Diatom-Symposium. Ottokoeltz, Konigstein, Germany. pp. 359-372.

.Stoerm(�r, E. F. 1984. Qualitative characteristics of phytoplankton assemblages.
Ed. L. E. Shubert. Algae as Ecological Indicators. Academic Press. New York,
New York. pp. 49-67.

Sullivan, M. J. 1986. Mathematical expression of diatom results: are these
"pollution indices" valid and useful? M. Ricard, Ed. Proceedings of 8th Diatom-
Symposium. Ottokoeltz, Konigstein, Germany. pp. 882-76.

U. S. Department of Agriculture. 1975. Special storm report: storm of April 10-
11, 1975. Choctawhatchee River basin, Alabama and Florida. Unpublished
report.

U.S. Study Commission. 1963. Plan for development of the land and water
resources of southeast river basins. Choctawhatchee-Perdido basins.

Wilderman, C. C. 1986. Techniques and results of an investigation into the
autecology of some.-major species of diatoms from the Severn River Estuary,

Chesapeake Bay, Maryland, U.S.A. M. Ricard, Ed. Proceedings of 8th Diatom-
Symposium. Ottokoeltz, Konigstein, Germany. pp. 631-643.

APPENDICES

Appendix 1: Sampling organization and protocols used during field operations
in the Choctawhatchee River and Bay system and offshore areas of the
Gulf of Mexico.

Appendix II: Quality Assurance and Quality Control protocols and Standard
Operating Procedures used during the Choctawhatchee field programs.

Appendix III: Photographic atlas of dominant phytoplankton species found in the
Choctawhatchee Bay system.

APPENDIX I

CHOCTAWHATCHEE RIVER AND BAY SYSTEM
AND ASSOCIATED GULF AREAS

SAMPLING ORGANIZATION
AND PROTOCOLS

Robert J. Livingston
Center for Aquatic Research
and Resource Management
Florida State University
Tallahassee, Florida 32306

CHOCTAWHATCHEE RIVER STATIONS
FIELD SAMPLING PROGRAM

STA. WAT.QUAL NUTRIENTS SF=DIMENTS PHYTOPLANKTON
Guaged station
60S
(Pine Log
Creek) x x x x

*61 S
(Choctaw-
hatchee R. x x x x

62
(Seven Run
Creek) x x x x

*63
(Choctaw-
hatchee R. x X. x x
Discontinued 3/87)

64
(Bruce Cr.). x x x x

65S
(Holmes
Creek) x x x x

*66
(Choctaw-
hatchee R. x x x x
disco ntinued3/87)

67S
(Sandy Cr.) x X. x

*68S
(Choctaw-
hatchee R.) x x x x

69S
(Wright's
Creek) x x x x

*70S
(Choctaw-
hatchee R.) x x x x

Station 68
Caryville

Station 68 is located near Caryville, where US-90 crosses the
Choctawhatchee River. The site is about 500 m in length and 150 m wide. Both
banks are steep with much snag habitat. There are areas of overhanging
willows on both upstream banks. The shoreline is sandy underneath the US-90
and railroad bridges. There is a granite breakwater located just north of the
railroad bridge. The surrounding forest is primarily oak, gum, tupelo, and other
floodplain species. There is no submergent or emergent vegetation. The water
is usually turbid.

Station 69
Wright's Creek

Station 69 is located approximately 10 k northwest of Bonifay on SR-1 77.
The site is about 75 m in length and 10 wide. The upstream area is narrower,
has steep banks, and is surrounded by dense old growth forest. The banks are
mostly' snaggy habitat with several large trees lying in midchannel. The
downstream right side is characterized bya large limestone outcropping and
sand-clay beaches. There is ar large cove where the water flow is usually slow.
The right bank is steep with much scrub. The channel narrows considerably at
the downstream end of the station and forms a shallow, pebbly riffle area with
accelerated water flow. The area surrounding the downstream portions of the
station is mostly flat and grassy. There is no emergent or submergent
vegetation. The water is usually clear. Brook salamanders (Eurycea) were
common.

Station 70
Pittman

Station 70 is located approximately 5 k west of Pittman on SR-2. The
station is about 500 k in length and 150 m wide. The banks,on both sides are
very steep and high (bluff-like), and covered with old growth and floodplain
forests. The upstream left side is mostly snag habitat with several large
submerged trees. The downstream left side has a shallow cove with sandy and
vegetated (maidencane) beaches, and a large stretch of overhanging willows..
The upstream right side is mostly scrub and snag habitat. Midstream on the
right side is an extensive limestone outcropping. The extreme downstream right
side of the channel is snag habitat. The channel along the right side is very
deep. The channel is shallow and sandy, with numerous sand bars, on the
upstream half of the station. The water is usually turbid.

Station 64
Bruce Creek

Station 64 is approximately 3 k downstream from SR-81 (which is about
8 k south of 1-10). The site is about 75 m in length and 10 m wide. This station
is characterized by,numerous large fallen trees and extensive snag habitat
along both banks. The channel is deep except in a clay and pebble riffle area
at the downstream end. The left bank is steep and primarily clay. The right
bank is steep at the upstream and downstream ends and gently sloping in the
middle. There is much clay and organic debris on the right bank. The forests
surrounding this tributary are primarily oak, magnolia, and pine, with some
scrub (primarily cabbage palm). The entire channel is overhung by a fairly thick
canopy. There is no submergent or emergent vegetation at this station. The
water is usually clear.

Station 65
Holmes Creek

Station 65 is located at SR-79 near Verno n. The site is approximately
500 rn long and 25 rn wide. The sides are mostly snag habitats. There are
many large fallen trees and submerged pier pilings. The left side is primarily
deep, with many complex root habitats, and patches of emergent and
submergent vegetation. There is a large cypress-bordered cove on the left side.
The right side is also deep, with steep limestone banks, and sloping forested
banks. The forests on both sides of the site are primarily old growth hardwoods
with thick overhanging canopies in places. The middle of the channel is mostly
deep sandy bottom, interspersed with several large sand bar areas. These
shallow areas are covered with submergent vegetation. The water is usually
clear.

Station 67
Sandy Creek

Station 67 is located behind the 1-10 and S R-81 rest area. The site is
about 75 m in length and 15 rn wide. It is mostly shallow, sandy riffle area.
Some deep areas have developed (via scouring) in the channel in the proximity
of large fallen trees. Both banks are mostly snag habitat, with large patches of
scrubby and sandy areas on the left side. The banks are moderately steep and
sandy. There is a large patch of submergent vegetation (Ludwigia, Egeria and
Nasturtium) near the left bank. The surrounding forest is mostly old growth
hardwoods and pine. The water is usually clear. A wild goat was observed.

Station 60
Pine Log Creek

Station 60 is located approximately 3 k south of Ebro on SR-79. The
sample site is about 75 m in length and 10 m wide. The upstream portion of the
site is bounded by thick strands of young pine and scrub oak. The upstream
rbanks are characterized by a mixture of snags, roots, and scrubby bushes. The
downstream banks are covered with scrubs and the surrounding shorelines are
mostly grass. Both banks are steep. There is no submergent or emergent
vegetation at this site. The middle of the channel is primarily shallow, sandy
riffle areas with deep spots at both ends of the station. The right bank is clay
underneath the SR-79 bridge. The water is usually darkly stained. Mice
(Peromyscus), water snakes (Nerodia), and skinks (Eumeces) were commonly
found along the scrubby shoreline.

Station 61
Ebro

Station 61 is located approximately 3 k west of Ebro on SR-20. The area
sampled is about 500 m long and 150 m wide. Both sides of the channel are
mostly high, steep banks (bluff-like). However, there are sandy (left side) and
forested areas (right side) of low, gently sloping shoreline (downstream of the
SR-20 bridge). The forests surrounding the river at this site are comprised of
oaks and pine (left side, downstream); cypress and bay (inside fish camp
channel); willows (portions of the left and right sides, upstream); and bay,
tupelo, river hickory and oak mixtures (upstream, right). The right shoreline is
predominantly snag habitat (snags, roots, and large fallen trees). There is a
small strand of overhanging willows on the upstream right side. The left
shoreline is characterized by large stretches of sandy beach (midstream and
downstream), a large area of overhanging willows (upstream), and large areas
of snag habitat (upstream and downstream). There is no submergent or
emergent vegetation. The water is usually turbid. Water snakes and alligators
(Alligator mississippiens) were observed at this station.

Station 62
Seven Runs Creek

Station 62 is approximately 24 k south of 1-10 on SR-81. The site is
approximately 75 m in length and 10 m wide. The left side and upstream right
side are bordered by thick strands of young oak. The far upstream portion of the
station has a thick overhanging canopy. The left side of the channel is gently
sloping and has large submerged leaf banks and patches of emergent
vegetation (maidencane). Both sides have patches of submergent grasses
(Vallisneria and Sagittaria) downstream. The right side of the channel is steep
and comprised mostly of dense scrub and snag habitat. There is an old
concrete pier in the middle of the channel. The water varies from clear to
moderately stained. Alabama wat.erdogs (Necturus alabamensis), Amphiuma
(Amphiuma), and three-lined salamanders (Eurycea longicauda guttolineata)
were frequently observed in the leaf banks.

CHOCTAWHATCHEE BAY SYSTEM
FIELD SAMPLING PROGRAM

A. Physical - chemical Analysis

1. Basic water quality and nutrients

temperature nitrate
pH nitrate
dissolved oxygen total Kjeldahl nitrogen
color ammonia
turbidity orthophosphate
secchi depth total phosphorous
salinity chlorophyll (a,b,c)
particulate organic matter (POM)
and carbon (POC)

The above parameters will be evaluated monthly from surface and bottom water samples at each of the

46 stations. In addition, chemical oxygen demand and coliform bacteria (fecal, total) will be determined

for the river and bayou sites. The 24 hour surveys will include measurements of temperature, salinity, and

dissolved oxygen. Such observations will be made at 4 hours intervals and at 1 meter depth increments.

2. Sediments

Basic data, including particle size distribution and percent organics, is to be taken quarterly at all

46 stations. Auxiliary information will include depth profiles of Eh, pH, dissolved oxygen, salinty,

temperature, and nutrients. Spatial and temporal scope of this additional work is yet to be determined. We

have an agreement with the Florida Department of Environmental Regulation that quantitative metal analyses

will be provided for three of our stations.

B. Plankton

ichthyoplankton (505 micron mesh net)
zooplankton (202 micron)
meroplankton (80 micron)

Surface samples will be obtained durng the day in duplicate nets
at 10 stations each month for each net type. Samples will be taken at
the mid-bay station of each of the 10 transects and a set of data will
be taken in Old Pass Lagoon (Station 36). At the 24 hour study sites
both day and night samples will be obtained, where samples will be taken
at the surface (nets), mid-depth (pump), and bottom (pump).

C. Fishes and invertebrates

Epibenthic fishes and invertebrates--seven two minute trawl tows
monthly at all transect stations (32 sites). Two two-minute trawl tows
will be taken at selected bayou stations and the Choctawhatchee River
station.

Infaunal macroinvertebrates--10 cores (3" diameter) monthly at all
transect stations (32 sites) and the Choctawhatchee River Station.
Cores will be processed through a 500 um mesh sieve.

Additional fish samples--trammel nets, gill nets, and lift net
samples will be obtained at five 24 hour stations each month. Exact net
deployment (location, duration, etc.) will be at discretion of chief
scientist, Dr. Christopher C. Koenig. Fishes too large to be returned
to the laboratory will be identified and measured in the field.
Stomachs will be removed and preserved and selected specimens will also
have gonads removed.

D. Addiitonal studies

1. seagrasses-A review will be made of the historic changes
of emergent and submergent vegetation in the
Choctawhatchee Bay system. This will be carried out
largely with aerial photographs. By spring, 1986,

an experimental program will be established (based
on the background data and historical reviews) which
will include transplant experiments with seagrasses
in an effort to enhance the productivity of this
area. Data will be generated concerning standing
crop biomass and productivity of existing beds with
an emphasis on stations 26, 26A, 35, 37, 39, and 42.

2. Oysters-stations 16 and 17 will be analyzed for various
factors associated with oyster propagation in the
estuary. These data will be compared with ongoing
studies by the Florida Department of Natural Resources.

All field work will be carried out using a fleet of boats from
Florida State University with an estimated sampling time of 5-7 days.
Such sampling will be performed during the third week of each month
(weather permitting) over a 12 month period starting in September, 1985.
Data generated will be placed in computer files for analysis with
CARRMA'S software system and computers located in the Florida State
University Computing Center. At the same time, a modeling program will
be developed in conjunction with water qualitymodels developed by the
Northwest Florida Water Management District. As soon as all data have
been entered (October, 1986), a series of model runs will be made using
different management scenarios with application to predictions of the
response of the Choctawhatchee Bay system to proposed structural
modifications.

II SAMPLING SUMMARY BY STATION

WQ--basic water quality and nutrients
24-H--24 hour vertical profiles (temperature, salinity, DO)
CC--chemical oxygen demand and coliforms
PKT--plankton samples (D=day only, D/N= day and night)
7TR--seven trawl tows, epibenthic fishes and invertebrates
2TR---two trawl tows
CORE--benthos (core samples), infaunal macroinvertebrates
AUX NETS--auxiliary nets (trammel, siene, gill, lift)
SED--sediments
SG--seagrasses
0YS--oysters

Station Data Type
AUX
WO 24-H CC PKT 7TR 2TR CORE NETS SED SG OYS

1 (Choc. River) X X X X X

2 X X X X

3 X D X X X

4 X X X X

5 (LeGrange bayou) X X X X

6 X X X X

7 (night stop) X X D/N X X X X

8 X X X X

9 (Alaqua bayou) X X X X

10 X X X X

11 X D X X

12 X X X X

13 (Basin bayou) X X X X

14 X X X X

15 (night stop) X X D/N X X X X

16 X X X X X

17 (Hogtown bayou) X X X X X

18 X X X X

19 X D X X X

AUX
X,'->TR CORE
WQ 247H CC F,[.-*.:T 7TR NETS SED SG OYS
InC
x x x x

v
/% x x x

x D x x x

2 3 x x x x

24 x x x x

24A
A x x x

25 (night stop) x x D/N X x x x

26 x x x x x

26A x x x x x

27 (Rocky bayou) x x x x

x x

29 (Boggy bayou) x x x

x x x x

I (night stop) x x D/N X x x x

-12
A x x x

x x x

34 x D x x x

35 x x x x

36 (Old Pass Lagoon) X x D x x

7 x x x x x

38 (night stop) x x D/N X x x x

-zg x x x x x

4(--) (Garnier bayou) x x x x

41 (Cinco bayou) x x x x

42 x x x

4 -3. (the nar-r-ovis) x x x

44 (open Gul-r) x x

III. PROTOCOLS (FIELD SAMPLING AND ANALYSIS)

A. Physical-chemical parameters

1. Water Quality Data

Field meters and equipment will be used on site for,

Temperature
PH
D.O.
Secchi
Sa1inity
Chlorophyll--filter 10 L on site

Field efforts at each station will consist of taking eight samples,

each to be preserved according to protocol. One of these samples

will be a quarterly sediment sample. COD and Coliform samples will be

taken at designated fresh water input points of the bay.

2. Protocol for Chemical Sampling Choctawhatchee Bay

Coliform bacteria will be collected in sterile plastic bags.
A sterile plastic bag will be filled beneath the surface of the water;
a sweeping motion will be used with the open end of the bag kept
towards the sweep. For depth, bags will be filled directly from the
Kemmerer bottles. Samples will be immediately placed on ice.

TKN samples will be taken and acidified at the rate of 0.8 ml HzSO4/L
and kept at 4-C in I L glass containers. Containers will be washed out
with sample water and then filled from Kemmerer sampler or directly from
Surface waters.

Total P, PO4 Nitrate ammonia samples will be taken in 1L polyethelene
containers. Containers will be washed out with sample water and samples
will be taken from Kemmerer bottles or directly from Surface waters.
These samples will be analysed or frozen immediately.

Nitrite will be sampled from Kemmerer bottles in 500 ml polyethelene
containers. Containers will be washed out with sample water before
sample is taken. Samples will then be analysed or frozen immediately.

COD, color and tUrbiditv will be taken in 500 ml polyethelene containers
that have been washed out with sample water and then placed immediately
on ice.

POC and POM will be collected in I I polyethelene containers, after
washing containers with sample water. They will then be analysed or
frozen immediately.

Sediments will be taken quarterly in 1000 ml coring containers and kept
at 4 C

Chlorophyll will be taken by filtering 10 1 of sample water and staring
filters at -2 C or will be analysed immediately.

3. Chemistry Methods Choctawhatchee Bay

Nitrogen (ammonia)--Nesslerization, measurement spectrophotometric at
425nm.

Ni t r o g e n(nitrate)--Reduction, diazotization, measurement
spectrophotometric at 400 nm.

Nitrgen(nitrite)--Diazotization. Measurement spectrophotometric at 505
nm.

Phosphorous total )--Acid hydrolysis, persulfate oxidation. Measurement
spectrophotometric at 880 nm.

Ortho-phosphate--Amino-naphthol reduction. Measurement
spectrophotometric at 880 nm.

Total Kjeldahl nitrogen--Hydroxide-thiosulfate-reagent digestion.
Measurement spectrophotometric at 400 nm-425 nm (0.4-
5mg/L) or with a 5 cm light path at 450 nm-500 nm (5-
60 ug/L).

Determination of Chlorophylls--Millipore filtering with addition of
MgCDs, extracted by acetone and spectophotometric
measurement at 730 nm, 664nm, and 630nm.

Determination of Particulate Organic Carbon---Filtering, then "wet
washing" with dichromate and conc. sulfuric acid.
Measurement spectrophotometric at 440nm.

PartiCUlate Organic Matter (POM- filter sample, dr
y for 24 hrs at
100cC, ash at 500-C for I hr.

Total and Feral Coliform---Hach MUltiple--tUbe fermentation technique, EPA
approved.

COD-EPA approved COD reactor, premixed reagents, with concentration
measured. by spectrophotometric means.

*All procedures EPA approved or adapted -from Standard Nethods for the
Examination of Water and Wastewater, Methods for Chemical Analysis of
Water and Wastes (American PUblic Health Association, APHA) and a
ManUal of Chemical and Biological Methods -for Seawater Analysis
(Pergamon Press, 1984).

B. Protocol for Plankton Sampling

General Procedures:

Attach nets to frame securely

Set flowmeter setting to Zero or record initial flowmeter reading.

Check cod ends to make sure they are SeCUrely attached.

Launch nets.

Tow for specified time period at towing speed of 1-1.5 m/sec (2-3
knots)

Retrieve nets.

Record time of towing, boatspeed, flowmeter readinG time of day,
tidal stage, depth, kind of TOW.

Wash sides of net, then remove cod End, pour sample into prelabeled
bottle, pour preservative (Approximately 1 : 100), seal, and
store .

Specific procedures

phytoplankton Sampling- Nannoplankton
Using Kemmerer Bottle obtain 50O ml of water/sample.
Preserve with 5 ml LugOl'S Solution.

Phytoplankton Sampling - Net plankton
Tow 6o um net for 2 min (*Less if net is obviously no
longer filtering water)
Preserve with 5 ml Lugol's Solution

Meroplankton Sampling

Tow 80 um net for 2 min. (less if not filtering at end)
Preserve with 2-3 ml Buffered formalin.

Zooplankton Sampling:

Tow 202 um net for 10 min.
Preserve with 2-3 ml Bufferred formalin.

Icthyoplankton Sampling:

Tow 505 um net for 10 min.
Preserve with 2-3 ml Buffered formalin.
When all sampling the day is done wash all nets down with
freshwater.

This will help keep the nets in good condition- do not wait until the
next day since the corrosive effects of the sea water will already be
affecting the nets.

Keep all nets out Of the way during other sampling and put away and out
Of the sun as soon as possible.

Plankton Pumping Protocol

1. Begin pumping water at desired depth (use hose/marked at
.25 m increments)

2. Place graduated (in liters) bucket under hose nozzle and
Measure time to fill to obtain pumping rate.

3. Place hose above plankton net and pump for appropriate time
(pumping rate x time = Volume).

4. Remove hose, remove cod end of not and remove sample.

5. Replace cod end and pump again for 2nd sample.

6. Preserve sample with appropriate preservative.

Notes for calculation of sampling volumes for towed plankton samples:

[volume = d' x N x A ]
(i n

Where d' = calibration factor for flow meter. This factor
is generally between .15 and .16. It should be
listed on technical material from Supplier. it
can also be calculated iF distance towed is
known (d' = D/N)

N = Number of revolutions of flowmeter

A Area of the net mouth in meter2

A = r2

A B" net - .0183 m2 (r=.0762m r2=.0058m2)

A 20" net .2033m2 (r=. 2540m r2=.0645m2)

Suggested Volumes (EPA) 1.5-5m3

1m3=1000 liters

Plankton Towing Depth Calculation

Depth = L x cosine towing angle
Where L= length of line

C. Fish and Invertebrates

1. Protocol: Fish collection methods

1) Trawl ing: A standard 16 ft. otter trawl (try net)
designed for biological sampling will be used to
collect epibenthic fishes and macroinvertebrates.
Seven 2 min. tows will be made at each designated
station. Each tow should cover approximately 100
meters of bottom which means that tow speed should
be about 1.85 mph.(3.0KM/HR). Scope on the trawling
line should be about 7.1; thus, for Choctawhatchee Bay,

2) Beach Seining: A 50 ft. 1/4 in. mesh beach seine will be
used to collect near-shore fishes and invertebrates.
Three consecutive 33 meter tows will be made with the
lONG-shore current in areas conducive to this type of
collecting (i.e., sandy beach areas) close to designated
stations.

3) Trammel net collecting: A 100 meter trammel net (1 1/2
in. inside mash, 12 in. outside mesh) will be used to
collect bottom, midwater and surface dwelling fishes.
The trammel net will not be fished convertionally. By
the addition of leads and floats to the end thirds of the
net, one third will fish midwater, and one third will
fish the surface. The net will be set at designated
stations at dusk and fished for about 4 hours. The net
must be marked with flashing lights at night.

4) Night lighting: Fishes will be collected at night off the
R/V Nectes by use Of a 500 watt quartz flood light and
several fishing methods: a) dipnet, b) lift net and c)
small mesh gillnet. Dipnets will be operated by hand,
lift-nets (1/8" mesh) will be suspended about 1 meter
below the Surface directly beneath the floodlight. The
net will be lifted by hand when fishes have accumulated
under the light. The sample mesh gillnets 1/2"-3/4"
square mesh will be fished for four hours off the stern
from 12 ft. poles suspended near the surface.

Coring: General protocol for macroinvertebrate coring

1. Take 10 cores (5.5cm diamerter-10cm depth) per station.

2. Gently sieve each core through a 500 cm screen with sea water.

3. Wash material retained on screen into 32 oz. plastic
jar and add:
1-2ml Rose Bengal soultion *
2-3ml Formaldehyde*

4. Double check labels and store sample.

*Since all samples; are being sieved in the field, only small
quantities of Rose Bengal and Formaldehyde will be necessary
to insure adequate straining and fixation.

D. Trophic (Food web) analyses

Protocol: procedure for fish preservation and stomach content
analysis

1 . Fishes Must be fixed in 10% buffered formalin (Sat. sodium borate-formalin).

a) fishes smaller than ca. 7cm SL can be preserved whole
without opening body cavity.
b) fishes larger than 7 cm SL must be slit along the body
cavity too expose the stomach to the formalin Solution.
c) fishes too large to preserve should be weighed and
measured (SL) and stomach and gonad removed and preserved
in 10% buffered formalin.
d) preserved fish samples should be identified by waterproof
labels inserted in the jars with the fish. Included on
the label should be date, station number and method of
collection. Written with pencil.

2. Fishes held in formalin for at least a week should be washed
out in tapwater (allow several rinses of sufficient duration
to remove formalin) and stored in either 50% isopropyl alcohol
or 7% ethyl alcohol.

Weigh (gm) and measure (mm) fishes prior to removing stomachs.
Use standard length (SL) on all bony fishes (straight line
distance from tip of upper jaw to end of hypural plate).
Measure total length (TL) of sharks and disc width of rays.

4. Remove stomachs and collect contents in vials with 70% ethyl
alcohol and rose bengal.
a Pool stomach contents of smaller fishes of the same
species and size class (CA. 10-15 stomachs depending on
quantity of contents).
b) Determine stomach contents of larger fishes separately.

5. Transfer stomach contents to a series of nested sieves (2.0 mm,
0.850mm,0.425mm,0.250mm,0.125mm,0.075mm)and wash contents
through with an alcohol wash bottle or tap water.

6. Transfer each sieve fraction separately to small (CA. 2.5 in.)
culture dishes (or watch glasses) and count particles Of same
size class and identify proportion of different organisms
Under a stereo microscope.

7. Transfer each identified size class to aluminum weighing dishes
and dry at 60"'C. After a constant dry wt. is reached weigh
each fraction and record.

8. Calculate and record total dry wt. of stomach contents per fish
and the dry wt. of each of the identified portions. (some
classes may have to be identified as crustacean remains, shell
f ragments, etc.

9. Lori Wolfe should be consulted for a printout of the
identified stomach contents in 6) letter- codes.

Chemical parameters (of water and sediments) analyzed
in the Choctawhatchee River-Bay project

ORGANOCHLORINE PESTICIDES AND PCB'S CARBAMATES
(sediments) (water)
Aldrin Endrin aldehyde Aldicarb
arBHC Heptachlor Carbaryl
B--BHC Heptachlor epoxide
w-BHC Kepone Carbofuran
Methomyl
q:-BHC (lindane) Methoxychlor
Chlordane Toxaphene
4, 41 -DDD PCB-1016
4, 41 -DDE PCB-1221
43% 4' -DDT PCB-1232
Dieldrin PCB-1242
Endosulfan I PCB-1248
Endosulfan II PCB-1254
Endosulfan sulfate PCB-1260
Endrin Mirex

ORGANOPHOSPHORUS PESTICIDES CHLORINATED FUNGICIDE
(water) (water)
Azinphos methyl Merphos PCNB
Bolstar (Sulp rofos) Mevlnphos
Chlorpyrifos Monochrotophos
Coumaphos Naled
Demeton Parathion methyl
Diazinon Parathion
Dichlorvos Phorate
Dimethoate Ronnel,
Disulfoton Stirophos
(Tetrachlorvinphos)
EPN Sulfotepp
Ethoprop TEPP
Fensulfothion Tokuthion (Prothiofos)
Fenthion Trichloronate
Malathion.

METALS CHLORINATED-HERBICIDES OTHER HERBICIDES
(-sediments) (water) (water)

Aluminum 2, 4-D Trifluralin
Arsenic 2, 4-DB Benfluralin
Cadmium 2, 4, 5-T@ Metribuzin
Copper 2, 4, 5-TP Hexazinone
Chromium Dalapon
Iron Dicamba
Lead Dichloroptop
Mercury Dinoseb
Nickel MCPA
Zinc MCPP
Atrazine
Alachlor

OFFSHORE (GULF) STATIONS
OCTOBER, 1987: FEBRUARY, 1989

station Loran Reading

M-1 29:51:82N, 84:26:77W
M-2 29:49:47N, 84:26:19W
M-3 29:49:30N, 84:28:14W
M-4 29:39:72N, 84:25:59W

E-1 29:57:72N, 84:00:37W
E-2 29:51:25N, 84:04:96W
E-3 29:47:62N, 84:06:44W
E-4 29:41:79N, 84:10:05W

A-1 29:36:48N, 84:57:54W
A-2 29:31:48N, 84:54:49W
A-3 29:26:75N, 84:51:43W
A-4 29:20:39N, 84:48:05W

C-1 30:20:20N, 86:32:50W
C-2 30:15:30N, 86:32:90W
C-3 30:08:50N, 86:35:01 W
C-4 30:03:97N, 86:35:69W

APPENDIX 11

CHOCTAWHATCHEE RIVER AND BAY SYSTEM
AND ASSOCIATED GULF AREAS

QUALITY ASSURANCE/QUALITY CONTROL
AND
STANDARD OPERATING PROCEDURES

Robert J. Livingston
Center for Aquatic Research
and Resource Management
Florida State University
Tallahassee, Florida 32306

Quality Assurance Plan
for the
Choctawhatchee Project

Robert J. Livingston
Center tor Aquatic Research and Resource Management
Florida State University
Tallahassee, Florida 32306

Project Director

Associate Director

Consultant

Laboratory Director

Analyst

2. Contents

1) Title Page With Approval Signatures

2) Table of Contents

3) Project Description

4) Project Organization and Responsibility

5) QA Objectives for the measurement of Data

6) Sampling Procedures

7) Sample Custody

a) Field Sampling Operations

b) Laboratory Operations

8) Calibration Procedures and Frequency

9) Analytical Procedures-

10) Data Reduction, Validation, and Reporting

1 1 Field and Laboratory Quality Control Checks

12) Performance and System Audits

13) Preventive Maintenance

14) Specific Routine Procedures Used to Assess Data Precision,
Accuracy, and Completeness

15) Corrective Action

16) Quality Assurance Reports to Management

17) Personnel Qualifications, Resumes

3. Project Description
This project involves the monthly sampling of the water of the Choctawhatchee
River and its' tributaries. There are three main stem stations: 61 (Ebro), 68
(Caryville), and '70 (Pittman). There are six tributary stations: 60 (Piney, Log
Creek), 62 (Seven Runs Creek), 64 (Bruce Creek), 65 (Holmes Creek), 67 (Sandy
Creek),'and 69 (Wrights Creek). A map of the stations can be found in appendix 1.
Conductivity, pH, temperature and dissolved oxygen will be determined in the
field. Color, Turbidity, Biological Oxygen Demand, Chemical Oxygen Demand, Solids
(suspended, dissolved, fixed and volatile), Particulate Organic Matter, Total Organic
Carbon, Particulate Organic Carbon, Phosphate (dissolved, suspended, ortho and total),
Nitrate, Nitrite, and Kjeldahl Nitrogen (total and organic).
Data will be used to develop a model of the Choctawhatchee River. The chemistry
data will be combined with Hydrological data from the NWFWMD, and biological data
from our biologists to complete the model
Phase One of the project went from December to January 1987, Phase.Two of the
project goes from December to January 1988. There may be a Phase Three of the
project. In Phases One and Two 216 samples were taken. Nine per month for two years.
These samples were taken in duplicate, so we actually took 432 regular monthly
samples.
We also did Storm Monitoring, details of this program will be presented in
Appendix 2.

4. Project Organization and responsibility

R. J. Livingston (Proiect Direc1W

Glenn C. Woodsum (Associate Director)

S.E. McGlynn (Lab Director Jane Jimelan (Anaw

Hampton Hendry (Assistant) Rall2h A. Zuniaa (Assistant)

S. E. McGlynn and C Koenig (Field Team)

The Project D irector is the ultimate source of responsibility in this project. The
Project Director and Associate Director are responsible for all executive decisions
dealing with personnel, equipment, sampling sites, sampling intervals, parameters
monitored, methods, and final reports.
The Lab Director is responsible for implementing the policies of the Project
Director, receiving samples, directing analysis, stocking the laboratory, maintaining
equipment, updating the standard operating procedure, turning in all data to the analyst,
and performing the more demanding analyses. The Lab Director is the Quality Assurance
Officer.
The Analyst is responsible for all the raw data turned in by the Lab Director,
computing the finished data, filing the finished data, and reviewing the finished data with
.the Laboratory Director.
The Field Team collects the samples in the field and ships them to the laboratory.
They are responsible for the samples until they reach the laboratory, the Chain of
Custody forms, and the equipment while they are in the field.

5. Quality- Assurance Objectives
R METHOID- MATRIX PRECISION XrUWY COMPLET
PEK@ (%RSD) (sd) (%) - !n
Color 204B L 9 3 100
Conductivity 205 L 9 3 100
TIDS 209B L 12 50 100
TSS 209C L 12 10 100
POM&PIM 209D L 12 4 100
Salinity 21 OA L 9 3 100
Temperature 212 L 5 2 100
Turbidity 214A L 6 4 100
AlkalinitV 403 L 3 .5 100
Ammonia 417B L 6 .01 100
Nitrate 418C L 7 .05 100
Nitrite 419 L 6 .001 100
TKN&OKN 420B L 12 .2 100
D.O. 421F L 4 100
pH 423 L 5 .2 100
Phosphorus 424F L 7 .005 100
TOC 505A L 7 1 100
8M 507 L 7 1 100
OCD 508C L 17 5 100
Chlorophyll 4.1 t L 18 NA 100
*Unless stated otherwise methods are from Standard Methods for the Examination of
Water and Wastewater, 1985, 16th edition, APHA,AWWA, and WPCF.
t A Manual of Chemical and Biological Methods of Seawater Analysis, T. R. Parsons, Y.
Maita, and 0. Lalli, 1984, Pergamon P ress.

6. Sampling Procedures

"The result of any test can be no better than
the samples on which it is performed."
An old Axiom

The objective of sampling, is to collect a portion of material small enough in
volume to be transported conveniently and handled in the laboratory while still
accurately representing the material being sampled. This implies that the relative
proportions or concentrations of all pertinent components will be the same in the
samples as in the material being sampled and that the sample will be handled in such a
way that no significant changes in composition will occur before the tests are made.
. Sample bottles, usually half gallon plastic milk containers must be rinsed with
the water being sampled at least three times. Sample containers that are to be re-used
are washed with alconoxTm, rinsed at least three times with dl water, dried, and then
sealed to avoid any contamination. If phosphates are to be analyzed the sample containers
are acid washed with warm 10% HCI,.iand if trace metals are to be analyzed the sample
containers must be acid washed with 10% nitric acid.
Samples collected at a particular time and place can represent only the
composition of the source at that time and place. Grab samples are collected with a

Kemmerer sampler at the bottom of the water column. Composite samples are taken
with an integrated sampler. Avoid collecting detritus by taking the sample a few
centimeters above the soil/water interface. Surface samples are collected by lowering
an inverted sample container beneath the water/air interface and righting it. Avoid
collecting any flotsam and jetsam by filling the sample container 5cm beneath the
surface. Avoid entrapping air in the filled sample container. The sample must be
properly preserved until it is received at the laboratory.
When a source is known to vary with time, samples must be taken with
appropriate frequency to monitor the extent of these variations. In such a situation, the
location and the time of sample collection must be accurately duplicated. In open water,
a Loran can assure site location to within a hundred feet, otherwise landmarks must be
judiciously chosen.
Samples are put on ice in the dark immediately to assure stability of constituents
until they can be analyzed in the lab. Before delivery of the sample to the lab, a chain of
custody form must be filled out detailing the volume of the sample, the location of the
site, the date and time of sampling, the name of the samplers, the project'and/or the
parameters to be analyzed, the technique by which the sample was obtained, and the
methods of preservation. Completed chain of custody forms must be received and signed
by our laboratory personnel. Then they are filed at the laboratory where they are a
record of sample history. All subsequent tests performed on these samples are recorded
in the our Laboratory Log Book.
Samples are to be delivered to the lab with all possible haste, if delivery time
exceeds 6 hours, correct preservation techniques must be observed. IF these guidelines
,are observed samples on ice, with a proper chain of custody form will be accepted by the
laboratory. 'Once received samples are allowed to rise to ambient temperature before
analysis can begin.
The unequivocal preservation of samples is fundamentally impossible.
Regardless of the preservation technique, complete stability for every constituent can
never be achieved. It is best to analyze samples as soon as possible after collection, and
then to judiciously determine the type of preservation to be utilized.

Measurement Container Preservative Holding
Color P, G Cool, 4'C 48 hours
Conductance P, G Cool, 4'C 28 days
pH Pj G None None
Filterable Residue P, G Cool, 4'C 7 days
Non-filterable Residue P, G Cool, 4'C 7 days
Temperature P, G None None
Turbidit P, G Cool, 4'C 48 hours
Alkalinity P, G Cool, 4'C 14 days
Ammonia P, G Cool, 4'C, H2SO4 to pH < 2 28 dayL
Kieldahl Nitrogen P, G Cool, 4'C, H2SO4 to pH < 2 *28 days
Nitrate P, G Cool, 4C 48 hours
Nitrite P, G cool, 4'C 48 hours
Oxygen, dissolved P, G None None
Ortho-Phosphate G Cool, 4'C, no acid 48 hours
Total Phosphate G Cool, 4'C, H2SO4 to pH < 2 28 days
Phosphate, T. dissolved G Cool, 4'C, H2SO4 to pH < 2 24 hours
BOD P, G Cool, 4'C 48 hours
COD P, G Cool, 4'C, H2SO4 to pH < 2 28 days
Prganic Carbon P, G Cool, 4'C, H2SO4 to pH < 2 28 days

7. Sample Custody
Sample custody is important from a legal standpoint. We feel that it is
especially important that the great care taken in their work should be documented. No
time passes after the sample is taken without being documented. Chain of custody forms
cover the sample in the field, in transit, and in the laboratory. While in the laboratory
a log book charts the various analysis performed on the sample. . After all the
experimentation is complete the Chemist performing the analysis initials the original
Data Sheet. The original Data Sheets are handed to the Analyst by the Laboratory
Director. The original Data Sheets are filed'. The Data is punched into our Macintosh
Computer System by our Analyst and her assistants. After the Data is punched it is
checked by our Analyst who the initials the original Data Sheet signifying that it has been
checked. After calculations are performed on the Data it is stored on Bernoulli Disks.

a. Field Sampling Operations
Equipment that. goes in the field is prepared prior to each field trip. All field
meters are calibrated in the laboratory prior to each field trip. Typically, field crews
need a Salinometer, a Dissolved Oxygen Meter, a pH meter, and a thermometer.
The salinometer we use in the field is a YSI SCT Meter. It is calibrated against a
standard saline solution before each fibld trip. Usually if it does not calibrate the probe
must be cleaned with an HCI/isopropanol solution. The temperature sensor is calibrated

against an NBS thermometer. These methods are detailed in the YSI Operators Manual
(see SOP).
The dissolved oxygen meter we use in the field is a YSI DO Meter. It is Winkler
Calibrated quarterly. Before each field trip it is calibrated against an oxygen saturated
water solution. Before use in the field it is air calibrated. The DO Membrane is replaced
prior to use. If response is sluggish, or if there is any difficulty in calibration, clean
the silver electrode with a 14% Ammonium Hydroxide Solution, and clean th& gold
electrode with an abrasive rubber eraser.@ The temperature sensor is calibrated against
an NBS thermometer. These methods are detailed in the YSI Operators Manual (see SOP).
The pH meter we use in the field is a Corning 610 pH Meter. Of all our field
equipment this is the most prone to water damage. If it gets very wet the electronics
will be damaged. The calomel electrodes are kept filled with a saturated KCI solution. If
response gets sluggish clean the semipermeable membrane in warm pH 10 buffer, and
look for air bubbles in the ceramic junction. Before use the meter is calibrated to three
different pH buffers. The buffers are for pH 4, 7, and 10. These buffers are taken into
the field, and the meter is calibrated prior to each reading in the appropriate' pH range.
These methods are detailed in the Corning Operators Manual (see SOP).
The meters, a graduated depth line, and the Secchi must be signed out to the field
crew by the Laboratory Director, who makes sure all equipment is in full operating
condition.
The Field Crew labels all sample bottles after they have been cleared by the
Laboratory Director. The date, location, and station identification number must be
written on every sample bottle with a permanent marker. The Field Crew obtains Field
Data Sheets from the Analyst, it is the Analysts duty to work with the Project Director
and specify sampling locations and frequency, that are clearly stated on the Field Data
Sheets.
The Field Crew is responsible for custody of the sample until it is released to a
carrier or the laboratory. The chain of custody form initiated by the Field Crew states
the location, time, date, method of sampling, number of replicates, and method of
preservation of each sample. The persons in charge of the sample until it reaches the
laboratory must sign indicating the time when the sample came into their custody, and
when they relinquished the sample to someone else.

b. Laboratory Operations
The Laboratory Director is the sample custodian at the laboratory facility. He
signs for incoming samples and obtains documents of shipment. Once the samples arrive
at the laboratory their progress through analysis is documented in the Laboratory Log.
All analysis, new reagents, standard curves, etc. are signed and dated in this book by the
Chemist.
The Laboratory Director is responsible for the analysis of the sample. Results of
analysis are recorded on, the serially numbered Laboratory Data Sheets. These are a
complete record of the results of all the analysis performed on the samples from a given
field trip. The Laboratory Data Sheets also record the standards which are run. The
Laboratory Log details the observations and calibrations that may have occurred during
the run. It provides an accurate record of the date and time of each run, and of the
preservation status of any given sample.

8. Calibration Procedures and Frequency

Spectroph oto meters
(Bausch & Lomb Spectronic 2000, Beckman DB/G,
and a Carl Zeisse Elco 11)

A series of seven standards that bracket the range of concentrations anticipated
for any given parameter are run with every analysis as specified in our SOP. A standard
curve is generated from this data, and the slope and intercept are reported on the
original data sheet. If the R2 is less than- 0.90 the spectrophotometer is serviced and the
analysis is run again on a different instrument until a satisfactory calibration curve is
obtained.
All the calibration curves are kept on file by the Laboratory Director. Each new
Calibration Curve is compared by the Laboratory Director with previous Calibration
Curves from the same parameter. If there are significant differences between the
curves this is also cause for the analysis to be rerun.
All standards are made in our laboratory from ACS reagents according to EPA
specifications. 'A Stock solution is made first. The flask is dated and signed by the
Chemist who made it. A Standard solution is then made from the concentrated Stock
Solution. The flask is dated and signed by the Chemist who made it. Standards run with
the analysis are serial dilutions of the standard solution. They are made fresh for every
analysis.
All Stock and Standard solutions are recorded in our.Laboratory Log Book when
they are made. Old standards are discarded as they go bad. All the standards are dated.
We follow EPA guidelines in ascertaining their lifetime, and we check their age prior to
use. We also do a visual inspection of the standard before use. The ultimate test of the
standard is if it generates a good standard curve, however a bad standard curve can also
be caused by malfunctioning equipment.
We can trace our standards by checking in our Laboratory Log for the current
standard in use during any given analysis.

Mettler Balances
(Mettler H33, and a Mettler H15)
Our Mettler Balances are calibrated annually by certified. technicians. If there
are any problems with one of them we have a backup. With the, two balances we can
check the accuracy of one against the other.

Turbidometers
(2 Hach model 2100A)
These are calibrated with every use with commercial Hach standards as specified
in our SOP.

Colorimeters
(Hach DR-A, and a Hach DR-3)
These are calibrated with every use with commercial Hach standards as specified
in our SOP.

DO Meters
(3 YSI model 57)
These are air calibrated with every use. Winkler calibrated quarterly as
specified in our SOP.

SCT Meters
(3 YSI Model 33)
These are calibrated prior to each use with a standard saline solution as specified
in our SOP.

PH/mv Meters
(Beckman Century SS, and 3 Corning 610A)

These are calibrated with Buffered solutions obtained commercially at pH 4, 7
and 12. The mv scale used with an Ammonia sensitive Electrode is calibrated with the
seven point standards used for the Ammonia test as specified in our SOP.

9. Analytical Procedures
. Only EPA approved procedures are used in our laboratories.. All our laboratory
procedures are detailed in our Center for Aquatic Research and Resource Management
Standard Operating Procedures, (SOP).

10. Data Reduction, Validation, and Reporting
Only EPA approved procedures are used in our laboratories. All our formulas are
detailed in our Center for Aquatic Research and Resource Management Standard Operating
Procedures, (SOP).
All data is reported to our analyst. The Analyst and the Laboratory Director then
preliminarily validate the data, which is then sent to the project manager for final
validation. The criteria used to validate data integrity is adherence to our system of
absolute standards, the conformation of replicates to the %RSD as stated in section 6.5,
and the recovery of spiked samples from the field.

Data Flow

Project Director

Associate Director

Cohiputor System

Field Crew Analyst

Laboratory Director

11. Field and Laboratory Quality Control Checks
A random approach is taken as the basis of this statistical audit of our sampling
program. All sampling in rthe field is done in triplicate. From these triplicate samples
our replicate analysis are performed.
We run 10% replicates, on every analysis performed in our laboratory.
Replicates are reported on the Data Sheets turned in to the Analyst. It is left to the
discretion of the Chemist to perform replicates within the necessary 10% framework.
We expect all replicates to correspond to our Quality Assurance Objectives detailed in
section 5. If they do not corrective action is outlined in section 15.
Every sampling we undertake gets at least one spiked field sample for each
parameter analyzed. We run a field blank along with our field spikes. If a project
continues over a period of time spiking is repeated with each sampling mission. Field
Spikes are usually performed on the natural water being tested. If there is any
particular quality of the water that would interfere with our analysis this should help
make it apparent. The natural value of this parameter. will have to be analyzed in our
lab and then subtracted from the spike. We expect 95% recovery of all spikes. The
results of our Field Spikes are kept on file by the Quality Assurance Officer, and are
reported in our quarterly Quality Control Report to the Project Director.
Equipment Blanks and Calibration S 'tandards are employed with every run of our
laboratory equipment. From the results a calibration curve is calculated in our
StatviewTm Program. These are kept on file by the Quality Assurance Officer, and are
also reported on the Data Sheet turned in to the Analyst.
Surrogate samples are sent to us annually by cooperating labs in the area.
Analysis is performed on these samples as if they were Spikes. The Chemist does not
know the concentrations of the parameters he is testing for. We expect 95% recovery of
all surrogate samples. The results of our Surrogate Sampling are kept on file by the
Laboratory Director, and are reported'in our End of the Year Quality Control Report to
the Project Director.

Many of the parameters that we test for have Alternate Methods of Analysis.
Alternate Analysis is performed whenever interferences may be occurring. The
Laboratory Director or the Project Director may request Alternate Testing at any time
they deem necessary. For example, we routinely run three alternate methods of
Ammonia analysis, the Nessler, the Phenate, and the Ion Sensitive Electrode methods.
All our reagents are made from ACS chemicals, and are stored according to
specifications. They are dated and signed by the chemist who makes them. They are
recorded in our Laboratory Log. They are kept on a computer inventory that is updated
quarterly by the Quality Assurance Officer. All outdated reagents are discarded
immediately. More importantly, since we run Equipment Blanks and Calibration
Standards with every analysis, we can tell from the results of our calibration curve if
our reagents are in good form.

12. Performance and System Audits
Inter-laboratory performance audits are a continuing ongoing endeavor in our
research. It is of fundamental importance that our data reflects the greatest possible
accuracy. Our equipment is thoroughly checked out each time it is used with a complete
set of calibration standards. Calibrations are performed at least once a month on all
equipment. If any instrument fails to calibrate we rely on the trained and certified staff
of Florida State University technicians in our Machine and Electronic Shops to repair the
equipment. Furthermore we submit to on site external equipment audits by DER on all
projects.

13. Preventive Maintenance
Preventive maintenance is the key to success in any experimental endeavor.
Properly performed it saves allot of time by minimizing down time of equipment. If
equipment does go down it is imperative to have back-up systems which can take over.
Field equipment needs the most preventive maintenance. All meters used In the
field needs to be cleaned thoroughly when they comes back to the laboratory. Field
probes need to be cleaned, their membranes need to be changed, and they need to be filled
with the appropriate fluids. When meters and probes go to the field all batteries need to
be checked. Then the instruments are calibrated to assure that they are working
properly. Two sets of meters and probes are always sent into the field so that we have
backups.
Laboratory equipment are maintained as follows. Balances-(two mettlers) are
protected from shock, and are cleaned after daily use. All maintenance, Quarterly
calibrations, are performed by certified personnel in our machine shop.
Spectrophotometers (two Bausch and Lomb, two Beckman DB/G, and a Zelsse) are
protected from liquid spills. They are cleaned (the optics) and calibrated with every
use. If they will not calibrated they are sent to our electronics shop were certified
technicians repair them. Ovens are cleaned after use and calibrated quarterly with a
NBS thermometer. Water traps are used with our vacuum pumps to protect them from
damage. Oil is replaced quarterly. Desiccators are kept freshly charged with dririte.
Colorimeters and Turbidometers are calibrated with every use, and their optics are kept
clean. All laboratory chemicals are dated, and the chemist that mixes them affixes his
name'to the bottle. The reagents are checked quarterly to make sure that they have not
gone bad.
If any equipment goes down we have backups for them. All are kept at optimum
working capacity so that they are ready to use when they are needed.

14. Specific Routine Procedures Used to Assess
Data Precision, Accuracy, and Completeness.
All samples are taken in triplicate. All analysis is performed with a minimum of
10% replicates. Every time samples come to the laboratory we require field spikes, and
,field blanks.
The spikes and blanks assure us that the sampling was performed correctly. A
good field blank which is devoid of the parameters analyzed shows that there was no
contamination of the samples. Field Spikes with a Percent Recovery above 90% shows
that there was no degradation of the sample before analysis. If the Percent Recovery is
below 90% corrective action must be taken.
All replicates are subjected to statistical analysis. The mean is calculated for
each pair of replicates are calculated as. follows:

Mean M = (X1 + X2)/2

The standard deviation is calculated for each set of replicates as follows:
Standard Deviation = S [I(X,-M)2 / (n-1 W/2

The Percent Relative Standard Deviation for each set of replicates is calculated as
follows:

Percent Relative standard Deviation% RSD = (S / M)(100%)

For any experimental analysis the mean Standard Deviation and the mean Percent
Relative Standard Deviation of all the replicates for a given parameter are calculated. If
it does not conform to the OA objectives of table 5 corrective action must be taken.

15. Corrective Action
The Percent Relative Standard Deviation and the Percent Recovery of Spikes are
the criterion on which will be based the possibility of corrective action. If the Percent
Relative Standard Deviation exceeds the values stated in section 5, or if the Percent
Recovery of Spikes is less than 90% the QA Officer shall notify the Project Director who
shall decide the course of corrective action.- Extremely high experimental values shall
also be brought to the attention of the Project Director by the QA officer.
The Project Director may decide that the data in question is worthless. If there
are mistakes in the calculations the Project Director will consult with the Data Analyst
(Jane Jimain), or if the experimental analysis is in question the Project Director will
consult with the Chemist (Sean McGlynn).
Corrective Action may also be initiated by the DER QA Office, Performance
Audits, System Audits, Laboratory/Interfield comparison Studies, or. QA project Audits
conducted by DER.

16. Quality Assurance Reports to Management
Quarterly Performance of Systems and Data Quality Reports will be submitted to
the Project Director by the Head Chemist (Sean McGlynn). These reports include:

A statistical assessment of Data the Percent Relative Standard
Deviation and completeness of analysis.
- Results of Performance Audits
- Results of Systems Audits
- Significant OA problems and recommended solutions
- The outcome of corrective actions
Copies of all QA reports are submitted to the DER OA office.

17. Personnel Qualifications, Resumes

Curriculum Vitae: Robert J. Livingston (March, 1989)
136b Conradi
Department of Biological Science -
Florida State University
Tallahassee, Florida 32306
Office: (904) 644-1466
Home: (904) 893-1453

Education

Princeton University - A.B. (1955-1959)
Columbia University - B.S. - equivalent (1961-1963)
Scripps Insitution of Oceanography (University of California, San Diego)
(1963)
Institute of Marine and Atmospheric Sciences (Univ. of Miami) - M.S., Ph.D.
(1964-1970)

Fellowships -and Honors

Undergraduate Fellowship - Princeton University
Graduated cum Laude, Princeton University
Dean's List - Columbia University
Aerojet-General Fellowship, Scripps Institution of Oceanography (U. of
California)
Robert E. Maytag Fellowship, Institute of Marine & Atmospheric Sciences
(Univ. of Miami)
Third Annual Conservator Award; Apalachicola Seafood Festival
Conservation, Award; Woodmen of the World, Life Insurance Society
Florida Scientist of the Year (1982); Museum of Science and Industry
(Tampa, Florida)

Academic and Research Positions

Research Aide (institute of Marine & Atmospheric Sciences; 1964)
Graduate Assistant (Institute of Marine & Atmospheric Sciences; 1967-1970)
Assistant Professor (Department of Biological Science, Florida State
University; 1970-1976)
Associate Professor (Department of Biological Science, Florida State
University; 1977-81)
Professor (Department of Biological Science, Florida State University;
1981 -present)
Director, Center for Aquatic Research and Resource Management (1984-
present)

Research Activities and Interests

The overall research effort of R. J. Livingston for the past 18 years
has involved continuous, long-term analyses of various river and coastal
systems with an emphasis on the north Florida Gulf Coast (Apalachee Bay,
Apalachicola Bay). Coupled with laboratory and field experimentation, this
work has included multidisciplinary systems analyses, population/community
structure, trophic interactions, and the impact of various forms of.
anthropogenous stress on physico-chemical and biological processes.
Currently, the research effort involves a comparison of 8 drainage systems
(Florida, Mississippi, Alabama, Georgia, South Carolina), experimental acology
of predator/prey relationships and the validation or verification of bioassay.
results with field data from rivers and coastal areas. The establishment of the
Center for Aquatic Research and Resource Management will provide a basis for
finalization of previous studies and the initiation of new directions for the
application of scientific research to resource management problems.

Ecological (field) study of Florida Bay and inshore waters of the Florida
Everglades (P.I., Dr. Durbin Tabb)
Acute toxicity studies of effects of Dieldrin on estuarine fishes of south
Florida (P.I., Dr. C. Richard Robins, Dr. Richard Wade)
Behavioral and ecological studies on circadian rhythms of reef fishes
(P.I., R. J. Livingston)
Studies on the long-term physiological effects of chlorinated hydro-
carbons and oil on estuarine organisms (P.I., R. J. Livingston)
Laboratory studies on the effects of inorganic mercury on fresh water
fishes (P.I., R. J. Livingston)
Field and laboratory studies on the impact of pulp mill effluents on
coastal organisms, Apalachee Bay (P.I., R. J. Livingston)
Field studies on the. effect of dredging and eutrophica'tion on areas of
Escambia Bay (P.I., R. J. Livingston)
Field and laboratory studies on the impact of pesticides on the behavior
and ecology of estuarine organisms, Apalachicola Bay (P.I.,
R. J. Livingston)
Ecosystems management and the application of scientific data to planned
development of estuarine and coastal systems (P.I., R. J. Livingston)
Field and laboratory studies concerning the effects of clearcutting and
storm water runoff on estuarine populations and communities (P.I.,
R. J. Livingston)
Analysis of recovery of bay systems previously affected by anthropogenous
disturbance with an emphasis on productivity, trophic structure and
community response (P.I., R. J. Livingston)
Ecosystern functions in coastal areas of north Florida (P.I., R. J. Livingston)
Trophic relationships of coastal species associations (P.I., R. J.
Livingston)
Comparison of the effects of pulp mill wastes on drainage systems in Florida,
Mississippi, Alabama, and South Carolina.
Experimental ecology and the validation concept.with respect to the impact

of toxic substances on aquatic systems. Dr. Livingston has been cho-
sen to lead a team from the E.P.A., the Virginia Institute of Marine
Science, and F.S.U. to test the validation hypothesis (P. I., R. J.
Livingston)
Validation of laboratory and field experimental data for 3 river systems in
the southeastern U. S. (P.I., R. J. Livingston)
Comparative analysis of long-term, multidisciplinary data in a series of
river-estuarine systems.
Ecosystem analysis of the Choctawhatchee River-Bay system.
Ecological studies of Lake Jackson, Florida.

Research Grants and Funding: R. J. Livingston, Principal
Investigator

F.S.U. COFRS: $5,000 (Effects of Inorganic and Organic Mercury on Fish
Physiology and Behavior; 1971-1973)
Florida Department of Transportation: $19,800 (Effects of Dredging and
Eutrophication on Escambia Bay)
National Oceanic and Atmospheric Administration (Sea Grant): $134,000
(Estuarine Analysis: Field and Laboratory Studies on Chronic Effects
of Pesticides and Other Pollutants on Estuarine Animals and
Communities; 1972-1974)
Florida Department of Pollution Control: $5,500 (Study of the Impact of
a Cattle Ranch on the Apalachicola Drainage System; 1973)
Board of County Commissioners, Franklin County: $57,000 (Physico-
chemical and Biological Analysis of Apalachicola Bay; 1972-1977)
Coastal Coordinating Council, Florida Department of Natural Resources:
$5,800 (Effects of Pulp Effluent on Apalachee Bay; 1972)
Buckeye Cellulose Corporation: $32,000 (Determination of Recovery of
Heavily Polluted Portions of Apalachee Bay after Cessation of Pulp
Mill Effluents; 1974-1975)
Buckeye Cellulose Corporation: $15,000 (Study of the Impact of the Storm
Water Runoff of a Clear-cut Area on the Apalachicola Drainage System;
1974-1975)
National Oceanic and Atmospheric Administration (Sea Grant): $80,000
Franklin County Board of County Commissioners: $24,000 (Energy
Relationships and Role of Dissolved Nutrients and Detritus in
the Productivity of the Apalachicola Drainage System; 1975-1976)
N.O.A.A. (Florida Sea Grant, with D.C. White) $73,506 (Impact of
Storm Water Runoff on Apalachicola Bay; 1977)
Environmental Protection Agency: $128,000 (Analysis of Statistical
Methods Used to Determine Effects of Pollutants on Aquatic Populations
and Species Assemblages; 1974-1976)
National Commission on Water Quality: $10,000 (As associate investigator
with Dr. Frederick Bell, Dept. of Economics) (An Assessment of the
Economic Benefits Which WijI Accrue from Incremental Improvements in
the Quality of Coastal Waters)
Florida Department of Environmental Regulation: $4,000 (Study of the

impact of Clearcutting on a Bay System; 1975)
General Development Corporation: $5,000 (Computerized Analysis of
Estuarine Data; 1977)
U.S. Environmental Protection Agency: $100,000 (Analysis of
Trophodynamic Processes, Apalachee Bay; 1977-78)
Buckeye Cellulose Corporation: $30,000 (Field 'and Laboratory Analysis of
Factors controlling Grassbed Productivity in Apalachicola Bay; 1978)
Florida Department of Environmental 'Regulation: $10,000 (Analysis of
Forestry Operations on Apalachicola Bay, 1978)
Franklin County Board of County Commissioners: $30,000 (Study of
Impact of Clearcutting; 1977-78) -
Eniviron,"nental Protection Agency: $6,000 (Ground Truth Data Supporting
Remote Sensing Analysis of Apalachicola Estuary; 1977-780
N.O.A.A. (Florida Sea Grant): $81,000 (Development of Models Concerning
long-term (8-year) Changes in the Biota of the Apalachicola Estuary;
1978-79)
Thompson Hayward Chemical Company: $24,000 (Life cycle toxicity tests;
long-term effects of dimilin on Fundulus heteroclitus; 1977-78)
National Science Foundation (Ecology Program, Washington, D.C.):'
$36,450 (with Drs. D. White, D. Simberloff, and D. Strong)
(Specialized Research Equipment Program, Instrumentation for
Biochemical Analysis in Ecosystems; 1978-79)
Franklin County Board of County Commissioners: $20,000 (Analysis of
Long-term Changes in the Physical, Chemical, and Biological Function of
the Apalachicola Bay System; 1980)
U. S. Department of State: Secretariat to the U. S. National Commission for
UNESCO: $3000 (Application of Scientific Data to Planning and
Management Processes; 1980)
U. S. National Science Foundation:, $3000. Secondary Science Training
Program, Lectures (1975-80)
Conservation Foundation (Washington, DC): $5000 (Use of Scientific Data
to Aid in Development of a Comprehensive Management Program for
Franklin County, Florida; 1980)
International Paper Company: $720,000. (Comparison of the impact of
paper mill discharges on drainage systems in Mississippi, Alabama, and
South Carolina; 1980-81)
.Coastal Plains Regional Commission (Florida Department of Community
Affairs): $25,000 (Apalachicola Critical Habitat Assessment)
N.O.A.A. (Florida Sea Grant): $90,000 and Franklin County Board of
Commissioners: $40,000 (Management Plan for the Apalachicola
Estuarine Sanctuary; 1981-82)
Coastal Plains Commission: $25,000, 1 year (Apalachicola Critical Habitat
Assessment; 1981)
N.O.A.A. (Florida Sea Grant and the Office of Coastal Zone Management):
$90,000, 2 years (Development of an Apalachicola Resource Atlas;
1981-82)
Franklin County Commission: $20,000 (Matching funds for N.O.A.A. grant;
1981-82).
Buckeye Cellulose Corporation: $7,000, 3 months (Review of information

concerning the Flint River in Georgia; 1982)
Florida Department of Environment Regulation: $15,000, 15 months
(Analysis of the impact of dredging on Apalachicola Bay; 1982-83)
U. S. Environmental Protection Agency: $1,200,000 (Field and Semi-field
Validation of Laboratory-derived Aquatic Test Systems; 1982-84) with
D. White and R. Diaz.
Franklin County Commission: $20,000 (Studies in the Apalachicola Bay
system; 1983)
U. S. Environmental Protection Agency: $380,000 (with W. Cooper,
Department of Chemistry) (Validation Studies in three river
systems of the southeastern U. S.; 1983-1985)
Philadelphia Academy of Natural Sciences: $37,800: (Ecosystem stu-
dies in the Flint River system, Georgia; 1983)
U. S. Environmental Protection Agency: $40,000 (Characterization of
offshore grassbeds in the Gulf of Mexico and as background for
offshore validation experiments; 1983-1984)
Florida Legislature through the Florida Department of Natural Resources and
the Franklin County Commission: $69,000 (Identification and analysis
of sources of pollution in the Apalachicola Bay system; 1983)
Florida Resources and Environmental Analysis Center: $6,800 (Water
quality/sediment analysis of Old Pass Lagoon, Destin, Florida; 1983-
1984)
Franklin County Board of Commissioners: $40,000 (Ecology of the
Apalachicola Oyster Beds; 1984-1986)
U. S. Environmental Protection Agency: $350,000 (with R. J. Diaz and
D. C. White) (Validation of estuarine microcosms and effects of
toxic substances on laboratory-field assemblages of
macroinvertebrates; 1984-85)
Man in the Biosphere Program, U. S. Department of State: $4000
(Computer analysis of long-term multidisciplinary field data; 1985-86)
Florida Legislature: $150,000 (Ecosystem analysis of the Choctawhatchee.
River-Bay system; 1985-86)
Florida Department of Environmental Regulation: $100,000 (impact of toxic
waste sites on rivers; 1985-86)
U.S. Environmental Protection Agency: $200,000 (with R. J. Diaz)
(Validation of, estuarine microcosms; 1985-86)
Florida State University: $150,000 (Establishment of the Center for
Aquatic Research and Resource Management; 1984-87)
U.S. Army Corps of Engineers: $9,500 (Analysis of salinity-defined popula-
tions in the Apalachicola estuary; 1985)
Florida State University (SRAD grant): $1,325 (Update of microcomputer
equipment)
Florida State University (summer research grant; COFRS): $1,500 (Analysis
of oyster data)
Florida Department of Environmental Regulation: $100,000 (Development of
a conference concerning The Rivers of Florida; 1986-87)
Florida Department of Community Affairs: $30,000 (Biological charac-
terization of Choctawhatchee Bay, Florida; Renaissance Plaza, Inc.,
grant; 1986-87)

Florida Department of Community Affairs: $30,000 (Continued field research
in Choctawhatchee Bay, Florida; 1987-88)
Northwest Florida Water Management District: $165,000 (Critical habitat
assessment of the Choctawhatchee River system; 1987-88)
National Oceanic and Atmospheric Administration: $9,416-00 (with Gary@
Ray) (Distribution of oyster larvae in Apalachicola Bay, Florida; 1986-87)
Florida Department of Environmental Regulation: $42,000 (Chemical
analysis of water and sediments of the Choctawhatchee River-Bay
system; 1987)
U.S. Environmental Protection Agency: $41,184 (Potential effects of long-
term climate changes in the southeastern U.S.; 1987-88)
Florida Department of Environmental Regulation: $5,991 (Atlas of diatoms
and other algal forms from selected drainage areas in central and
north Florida; 1987) with A. K. S. K. Prasad
Florida Department of Environmental Regulation: $100,000 (Continuation
funding for the center for aquatic research and resource management;
1987-88)
Northwest Florida Water Management District: $1,900 (Ranking matrix for
the water bodies of regional significance in northwest Florida; 1988
Caribbean Marine Research Center: $23,000 (Aquaculture support at the
FSU Marine Laboratory; 1988)
Northwest Florida Water Management District: $85,000 (Phase
11--Choctawhatchee River Basin Assessment; 1988-89)
U.S. Environmental Protection Agency: $5000 (Development of a river
model, 1988)
Florida Institute of Government: $30,000 (A simplified and rapid method for
assessing the biological disturbances resulting from stormwater and
marine discharges in estuaries, 1988-89)
Florida Department of Environmental Regulation: $19,970 (An Atlas of
Phytoplankton, 1988-89)
U. S. Department of State: $16,500 (Wetlands research in the N.E. Gulf of
. Mexico, 1988-89) .
Northwest Florida Water Management District: $85,000 (Choctawhatchee
River-Basin assess me nt-Phase 11, 1988-89)
Caribbean Marine Research Institute: $23,000 (Aquaculture support at the
FSU Marine Laboratory, 1989)
U. S. Department of Commerce, NOAA: $50,000 (Temperature/salinity
profiles of a series of gulf estuaries, 1989)

Reviewed Publications

1. A volumetric respirometer for long-term studies of small aquatic animals.
Livingston, R. J. 1968. J. Mar. Bio. Ass. U.K. 48: 485-497..

2. Acute and chronic effects of dieldrin on the sailfin mollie (Poecilia
latipinna). Lane, C. E., and R. J. Livingston. 1970. Trans. Amer. Fish.
Soc. 99(3): 389-395.

3. New design for the long-term respirometry of small aquatic animals.

Livingston, R. J. 1970. Copeia (4): 756-758.

4. Circadian rhythms in the respiration of eight species of cardinal fishes.
(Pisces: Apogonidae): Comparative analysis and adaptive significance.
Livingston, R. J. 1971. Marine Biology 9(3): 253-266.

5.. Synergism and modifying effects. Livingston, R. J., et al. 1974. (Marine
Technological Society, 1974) - Book Chapter (invited, in, Marine
Bioassays, Workshop Proceedings. U.S. Environmental Protection Agency).

6. Livingston, R. J., R. L. Iverson, R. H. Estabrook, V. E. Keys, John Taylor,
Jr. Major features of the Apalachicola Bay system: Physiography, biota, and
resource management. Florida Scientist 37(4): 245-271. 1974.

7. Hooks, T. A., K. L. Heck, and R. J. Livingston. 1975. An inshore manne
invertebrate community: Structure and habitat associations in the N.E. Gulf
of Mexico. Bulletin of Marine Science 26: 99-109.

8. Cripe, C. R., J. H. Cripe, and R. J. Livingston. 1975. An apparatus for
the quantitative determination of activity rhythms of aquatic organisms using
infra-red light emitting diodes. J. Fish. Res. Bd. Can. 32: 1884-1885.

9. Livingston, R. J. 1975. Impact of pulp mill effluents on estuarine and
coastal fishes (Apalachee Bay, Florida). Marine Biology 32: 19-48.

10. Zimmerman, M., and R. J. Livingston. 1976. The effects of Kraft mill
effluents on benthic macrophyte assemblages in a shallow bay system
(Apalachee Bay, North Florida, U.S.A.). Marine Biology 34: 297-312.

11. Livingston, R. J. 1976. Diurnal and seasonal fluctuations of estuarine
organisms in a north Florida estuary: Sampling strategy, community struc-
ture, and species diversity. Estuarine and Coastal Marine Science 4: 373-
400.

12. Koenig, C. C., R. J. Livingston, and C. R. Cripe. 1976. Blue crab mortality:
Interaction of temperature and DDT residues. Archives of Environmental
Contamination and Toxicology 4(l): 119-128.

13. Koenig, C. C., and R. J. Livingston. 1976. The embryological development
of the diamond killifish (Adinia xenica). Copeia(3): 435-445.

14. Livingston, R. J. 1976. Avoidance responses of estuarine organisms to
storm water runoff and pulp mill effluents. Invited paper, Proceedings of the
Third International Estuarine Research Federation conference, Galveston,
Texas. October, 1975. Estuarine Processes 1. 313-331.
15. Livingston, R. J. @ 106. Dynamics of organochlorine pesticides in'estuarine
systems and their *effects on estuarine biota. Invited paper, Proceedings of
the Third International Estuarine Research Federation Conference,Galveston

Texas. October, 1975. Estuarine Processes 1., 507-522.

16. Livingston, R. J. 1976. Time as a factor in environmental sampling popula-
tions and communities. Invited paper, Symposium on the Biological
Monitoring of Water Ecosystems (Ed. J. Cairns, Jr.). ASTM STP 607: 212-
234.

17. Livingston, R. J., G. Kobylinski, F. G. Lewis, and P. Sheridan. 1976.
Analysis of long-term fluctuations of estuarine fish and invertebrate popula-
tions in Apalachicola Bay. Fish. Bull. 74(2): 311-321.

18. Livingston, R. J., R. S. Lloyd., and M. S. Zimmerman. 1,976. Determination
of adequate sample size for collections of benthic macrophytes in polluted
and unpolluted coastal areas. Bull. Mar. Sci. 26(4): 569-575.

19. Zimmerman, M. S., and R. J. Livingston. 1976. Seasonality and physico-
chemical ranges of benthic macrophytes from a north Florida estuary
(Apalachee Bay). Contr. Mar. Sci. Univ. Texas 20: 33-45.

20. Livingston, R. J., et al. 1977. The biota of the Apalachicola Bay system:
Functional relationships. In, Proceedings of the Conference on the
Apalachicola Drainage System. Florida Marine Research Publications, Fla.
D. N. R. Eds., R. J. Livi ngston and E. A. Joyce, J r., Co nt. #26: 75-100.

21. Cripe, C. R., and R. J. Livingston. 1977. Dynamics of the pesticide mirex
and its photoproducts in a simulated marsh system. Arch. Env. Cont. Tox. 5:
295-303.

22. Lewis, F. G., III, and R. J. Livingston. 1977. Avoidance reactions of two
species of marine fishes of Kraft pulp mill effluent. Fish. Res. Bd. Can.
34: 568-570.

23. Livingston, R. J. 1977. Review of curr ent literature concerning the acute
and chronic effects of pesticides on aquatic organisms. Invited paper,
Critical Reviews in Environmental Control 7: 325-351.

24. Livingston, R. J., et al. 1978. Long-term variation of organochlorine resi-
dues and assemblages of epibenthic organisms in a shallow north Florida
(U.S.A.) estuary. Marine Biology 46: 355-372.

25. Laughlin, R. A., C. R. Cripe, and R. J. Livingston. 1978. Field and
laboratory avoidance reactions by blue crabs (Callinectes sapidus) to storm-
water runoff. Trans. Amer. Fish. Soc. 107: 78-86.

26. Stoner, A. W., and R. J. Livingston. 1978. Respiration, growth and food con-
version efficiency of pinfish (Lagodon rhomboides) exposed to sublethal con-
centrations of bleached Kraft mill.effluent. Env. Poll. 17: 207-218.

27. Meeter, D. A., and R. J. Livingston. 1978. Statistical methods applied to a

four-year multivariate study of a Florida estuarine system. Invited paper,
Biological Data in Water Pollution Assessment: Quantitative and Statistical
Analyses. American Society for Testing and Materials. Special technical
publication 652., Eds., John Cairns, Jr., K. Dickson, and R. J.
Livingston.
28. Livingston, R. J. 1978. Summary: Biological Data in Water Pollution
Assessment: Quantitative and Statistical Analyses. Special technical
publication 652, Editors: John Cairns, Jr., K. Dickson, R. J. Livingston.
American Society for Testing and Materials.

29. Livingston, R. J., (it al. 1978. Kepone/Mirex/Hexachlorocyclopentadiene:
An Environmental Assessment. Chairman, National Research Council Panel.
National Academy of Sciences.

30. Laughlin, R., R. J. Livingston, and R. Cripe. 1978. "Comments;" reply to
Reynolds and Casterlin concerning laboratory/field behavior of blue crabs.
Trans. Amer. Fish. Soc. 107(6): 868-871.

31. Livingston, R. J. 1979. Multiple factor interactions and stress in coastal
systems. A review of experimental approaches and field implications. In,
Marine Pollution: Functional Responses. Ed. F. John Vernberg.

32. Zimmerman, M. S., and R. J. Livingston. 1979. Dominance in benthic
macrophyte assemblages from a north Florida estuary (Apalachee Bay). Bull.
Mar. Sci_. 29, 27-40.

33. Livingston, R. J., and J. Duncan. 1979. Short- and long-term effects of
forestry operations on water quality and epibenthic assemblages of a north
Florida estuary. Ecological Processes in Coastal and Marine Systems, Ed..
R. J. Livingston.

34. Meeter, D. A., R. J. Livingston, and G. Woodsum. 1979. Short and long-term
hydrological cycles of the Apalachicola drainage system with application to
Gulf coastal populations. Ecological Processes in Coastal and Marine
Systems. Ed. R. J. Livingston.

35. White, D., R.*J. Livingston, et al. 1979. Effects of surface composition,
water column chemistry and time of exposure on the detrital microflora and
associated macrofauna in Apalachicola Bay, Florida. Ecological Processes
in Coastal and Marine Systems, Ed. R. J. Livingston.

36. Sheridan, P., and R. J . Livingston. 1979. Cyclic trophic relationships of
fishes in an unpolluted, river-dominated estuary in north Florida.
Ecological Processes in Coastal and Marine Systems, Ed. R. J. Livingston.

37. Livingston, R. J., and 0. Loucks. 1979. Productivity, trophic interactions,
and food web relationships in wetlands and associated systems. Invited
paper, Proceedings of the National Symposium on Wetlands. American

Water Resources Association.

38. Stoner, A. W., and R. J. Livingston. 1980. Distributional ecology and food
habits of the banded blenny, Paraclinus fasciatus: An inhabitant of a
mobile community. Marine Biology 56, 239-246.
39. Livingston, R. J. 1980. Ontogenetic trophic relationships and stress in a
coastal seagrass system in Florida. In,'Estuarine Perspectives, 423-436
(Academic Press).

40. Mahoney, B. M. S., and R. J. Livingston. 1982. Seasonal fluctuations of
benthic macrofauna in the Apalachicola estuary, Florida, U.S.A.: The role
of predation. Marine Biology 69, 207-213.

41. Livingston, R. J. 1981. Man's impact on the distribution and abundance of
sciaenid fishes. Sixth Annual Marine Recreational Fisheries Symposium;
Sciaenids: Territorial Demersal Resources. National Marine Fisheries
Service. Houston, Texas.

42. Livingston, R. J. 1981. River-derived input of detritus into the
Apalachicola estuary. Proceedings of the National Symposium on
Freshwater Inflow to Estuaries. U. S. Fish and Wildlife Service Publ.

43. Livingston, R. J. 1982. Trophic organization of fishes in a coastal
seagras s system. Marine Ecology, Progress Series, 7,1-12.

44. Livingston, R. J. 1982. Long-term variability in coastal systems:
background noise and environmental stress. In, Ecological Stress and the
New York Bight: Science and Management. U. S. Department of Commerce.
pp. 605-620.

45. Dugan, P. J., and R. J. Livingston. 1982. Long-term variation in macroin-
vertebrate communities in Apalachee Bay, Florida. Estuarine, Coastal and
Shelf Science 14, 391-403.

46. Greening, H. S., and R. J. Livingston. 1982. Diel variations in the struc-
ture of epibenthic macroinvertebrate communities of seagrass beds
(Apalachee Bay, Florida). Marine Ecology, Progress Series 7, 147-156.

47. Laughlin, R.. A., and R. J. Livingston. 1982. Environmental and trophic
determinants of the spatial/temporal distribution of the brief squid
(Lolliguncula brevis) in the Apalachicola estuary (North Florida, U.S.A.).
Bull. Mar. Sci. 32, 489-497.

48. Stoner, A. W., H. S. Greening, J. D. Ryan, and R. J. Livingston. 1982.
Comparison of macrobenthos collected with cores and suction dredge.
Estuaries 6, 76-82.

49. Federle, T. W., M. A. Hullar, R. J. Livingston, D. A. Meeter, and D. C.

White. 1982. Biochemical analysis of the spatial distribution, biomass,
and community composition of microbial assemblies in estuarine, mud flat
sediments. Appl. Environ. Microbiol. (June).
50. Clements, W. H., and R. J. Livingston. 1983. Overlap and Pollution induced
variability in the feeding habits of filefish (Pisces: Balistidae) in
Apalachee Bay, Florida. Copeia (1983), 331-338.

51. Sheridan, P. F., and R. J. Livingston. 1983. Abundance and seasona-
lity of infauna and epifauna inhabiting a Halodule wrightii meadow in
Apalachicola Bay, Florida. Estuaries 6, 407-419.

52. MacFarlane, B., and, R. J. Livingston. 1983. Effects of acidified water on
the locomotor behavior of the Gulf killifish. Arch. Env. Cont. Toxicol..
12,163-168.

53. Federle, T. W., M. A. Hullar, R. J. Livingston, D. A. Meeter, and
D. C. White. 1983. Spatial distribution of biochemical parameters indi-
cating biomass and community composition of microbial assemblies in
estuarine mud flat sediments. Appl. Env. Micro. 45, 58-63.

54. Livingston, R. J. 1983. Resource Atlas of the Apalachicola Estuary.
Published by Florida Sea Grant College and Florida Resources and
Environmental Service.Center.

55. Livingston, R. J. 1983. Research and resource planning in the
Apalachicola drainage system. Proceedings of the Apalachicola Oyster
Industry Conference, Apalachicola. Florida Sea Grant College.

56. Federle, T. W., R. J. Livingston, D. A. Meeter, and D. C. White. 1983.
Modifications of estuarine sedimentary microbiota by exclusion of epi-
benthic predators. J. Exp. Mar. Biol. Ecol. 73, 81-94.
57. Stoner, A. W., an d R. J. Livingston. 1984. Ontogenetic variation in diet
and feeding morphology in sympatric fishes of the family Sparidae from
seagrass meadows. Copeia, (1984), pp. 174-187.

58. Livingston, R. J. 1984. Trophic response of fishes to habitat
variability in coastal seagrass systems. Ecology 65, 1258-1275.

59. Livingston, R. J. 1984. Aquatic field monitoring and "meaningful"
measures of stress. Concepts in Marine Pollution Measurements. pp.
681-691.

60. Livingston, R. J. 1985. The ecology of the Apalachicola estuary.
Invited paper, U. S. Fish and Wildlife Series; Ecological Monograph.
61. Livingston, R. J. -1985. Organization of fishes in coastal seagrass
systems: the response to stress. In, Fish Community Ecology in Estuaries

and Coastal Lagoons. Ed., A. Yanez-Arancibia. Chapter 16:367-382.

62. Clements, W. E., and R. J. Livingston. 1984. Prey selectivity and iunc-
tional response of the fringed filefish, Monacanthus ciliatus (Pisces:
Monacanthidae). Mar. Ecol. Prog. Ser. 16, 291-295.

63. Livingston, R. J., and D. A. Meeter. 1985. Correspondence of labora-
tory and field results: What are the criteria for verification?
Proceedings of the Symposium for Multispecies Toxicity Testing. J.
Cairns, editor. Blackburg, Virginia. Chapter 8, pp. 76-88.

64. Livingston, R. J. 1985. -,The relationship of physical factors and
biological response in coastal seagrass meadows. Proceedings of a
Seagrass Symposium, Estuarine Research Foundation. Estuaries 7,
377-390.

65. Livingston, R. J. 1985. Aquatic field monitoring and meaningful measures
of stress. In: Concepts in Marine Pollution Measurements, Ed., H. H.
White. pp. 681-692.

66. Livingston, R. J., R. J. Diaz, and D. C. White. 1985. Field valida-
tion of labo ratory-de rived multispecies aquatic Test Ecosystems.
U.S.E.P.A., Research and Development Summary Paper.

67. Livingston, R. J. 1985. Application of scientific research to resource
management: Case history, the Apalachicola Bay system. Proceedings of
the international Symposium on Utilization of Coastal Ecosystems: Rio
Grande, Brazil. pp. 103-125.

68. Livingston, R. J. 1987. Historic trends of human impacts on seagrass
meadows in Florida (invited paper). Symposium Proceedings:
Subtropical-Tropical Seagrasses of the Southeastern U.S. Florida Marine
Research Publication 42:139-151.

69. Livingston, R. J. 1987. Field sampling in estuaries: The rela-
tionship of scale'to variability. Estuaries (Biological Variability in
Estuaries).

70. Livingston, R. J. 1986. Field verification of toxicity tests concerning
the impact of toxic waste sites on three southeastern drainage systems.
U.S.E.P.A., Research and Development Summary Paper.

71. Federle, T. W., R. J. Livingston, L. E. Wolfe, and D. C. White. 1986. A
quantitative comparison of microbial community structure of estuarine sedi-
ments for microcosms in the field. Can. J. Microbiology 32:319-325.

72. Livingston, R.. J. 1986 (invited paper, in press). Inshore marine habitats.
In: Ecosystems of Florida, eds. R. L. Myers and J. J. Ewel.

73. Livingston, R. J. 1988. Field verification of multispecies microcosms using
marine macroinvertebrates. American Society for Testing and Materials.
ASTM STP 971. pp. 369-383.

74. Livingston, R. J. 1987.Field verification of toxicity tests concerning the impact
of toxic waste sites on three southeastern drainage systems. U.S.E.P.A.
Research and Development Summary Paper.

75. Livingston, R. J. 1988.. Ecological processes of recruitment in coastal
epibenthic macrobiota: a comparative approach. Proceedings, IREP
Workshop on Recruitment in Tropical, Coastal, Demersal Communities.
Ciudad del Carmen, Mexico.

.76. Livingston, R. J. 1987. Scientific research and resource management:
Relationships and inconsistencies. Proceedings, National Wetland Assess.
Symposium. Portland, Maine, in press.

77. Livingston, R. J. 1988. Use of freshwater macroinvertebrate microcosms in
the impact evaluation of toxic wastes. Proceedings, A.S.T.M. Conference
(Bal Harbour, Florida). ASTM STP 998,166-218.

78. Livingston, R. J. 1988. Inadequacy of species-level designations for eco-
logical studies of coastal migratory fishes. Invited paper, Sixth Biennial
Conference on the Ecological and Evolutionary Ethology of Fishes.
Beaumont,Texas. Environmental Biology of Fishes, 22, 225-234.

79. Livingston, R. J. 1988 Environmental research: how much is enough?
Proc. Eighth Annual Minerals Management Symposium.

80. Livingston, R. J., and R. L. Howell, IV (in press). Effects of two hurri-
canes on oyster beds (Crassostrea virginica) in a gulf estuary. Estuaries

81. Ray, G. L., and R. J. Livingston (in press). The distribution of oyster
larvae in Apalachicola,Bay, Florida. Proc. Shellfisheries Association

82. Prasad, A. K. S K., R. J. Livingston, and J. A. Nienow (in press). The
.diatorn genus Cyclotella KQtzing (Bacillariophyceae) in Choctawhatchee Bay,
northeastern Gulf of Mexico: fine structure, taxonomy, and ecology.

83. Luckenback,. M. W., R. J. Diaz, C. C. Koenig, R. J. Livingston, G. L. Ray,
S. B.Thornton, and L. Wolfe (in review). Field validation of a multispe-
cies benthic microcosm. 1. An ecological guild approach.

84. Luckenback, M. W., R. J. Diaz, C. C. Koenig, R. J. Livingston, G. L. Ray, S.
B. Thornton, and L. Wolfe (in review). Field validation of a multispecies
benthic microcosm. 11. Response to pentachlorophenol.

85. Ray, G. L., and R. J. Livingston (in manuscript). The short-term dynamics
of estuarine polychaetes: (1) A comparison of oligohaline and polyhaline

populations.

86. Ray, G. L., and R. J. Livingston (in manuscript). The short-term dynamics
of estuarine polychaetes: (2) Interannual variation in a polyhaline popula-
tion.

87. Livingston, R. J. (in press, The Rivers of Florida). The Oklawaha River:
Environmental Overview.

88. Livingston, R. J. and Gary L. Ray. (in press, The Rivers of Florida). Ecology
of the alluvial rivers of Florida.

89. Livingston, R. J. and S. H. Wolfe. 1988. Restoration and Preservation Ranks
of Water Bodies within the Northwest Florida Water Management District.
Publication, Center for Aquatic Research and Resource Management

90. Livingston, R. J. 1986. Ecological processes of recruitment in coastal
epibenthic macrobiota. Proc., IOC/FAO Workshop on recruitment in
tropical coastal demersal communities. Report # 44, 151-166.

91. Livingston, R.J. (in press). Projected changes in estuarine conditions based
on models of long-term atmospheric alteration. U. S. E. P. A. publ. CR-
814608-01-0.

Other Publications

1. Living rhythms of the sea. R. J. Livingston. Sea Frontiers 14(5):
290-299. 1968.

2. Persistent pesticides and the aquatic environment. R. J. Livingston. Res.
Rept. Soc. Sci. 14(2): 7-10. 1972.

3. A sea water system designed for controlled experiments on the chronic
effects of pesticides on marine organisms. R. J. Livingston (with C. R.
Cripe, C. C. Koienig, A. J. Tolman, and B. D. DbGrove). Sea Grant
Publication, report #5, 1974.

4. Resource management and estuarine function with application to the
Apalachicola drainage system (North Florida, U.S.A.). R. J. Livingston.
Office of Water and Hazardous Materials, U.S. Environmental Protection
Agency: included in final collection of papers (reviewed and published for
submission to the Congress of the United States), Estuarine Pollution
Control and Assessment, Vol. 1, 3-17. 1975.

5. Translocation of mirex from sediments and its accumulation by the
hogchoker
Trinectes maculatus. .R. J. Livingston (with Gerard J. Kobylinski). Bul-
letin of Environmental Contamination and Toxicology 14(6): 692-698. 1975.

6. Environmental considerations and the management of barrier islands: St.
George Island and the Apalachicola Bay system. R. J. Livingston. Invited
paper, in Barrier Islands and Beaches. The Conservation Foundation.
Cont. V, 86-102. 1976.

7. Book Review: Marine Pollutant Transfer. R. J. Livingston. Science 198,
392. 1977.

8. Benthos, In: Oil Spill Studies. R. J. Livingston (with D. Boesch, C.
Hershner, K. Roos, D. Straughan, and A. Michael (Chairman and Editor)).
A.P.I. Publ. No. 4286, pp. 57-75. 1977.

9. The Apalachicola dilemma: wetlands development and management
R. J. Livingston. Invited paper, National Wetland Protection Symposium;
Environmental Law Institute and the Fish and Wildlife Service, U.S.
Department of the Interior. 163-177. 1977.

10. Estuarine and coastal research in Apalachee Bay and Apalachicola Bay. In
Coastal Zone Management Symposium, University of West Florida. 1977.

11. Book Review: Effects of Pollutants on Aquatic Organisms. R. J. Livingston.
Quart. Rev. Biol. 1978.

12. Book Review: Physiological Responses of Marine Biota to Pollutants.
R. J. Livingston. Quart. Rev. Biol. 1978.

13. Research, management, and the estuarine sanctuary concept: Where are
the ties that bind? Proceedings of the workshop on the National Estuarine
Sanctuary Program. The Georgia Conservancy, the Coastal Society. 1979.

1.4. Behavior workshop report: The role of Behavior in Marine Pollution
Monitoring (with Bori L. Olla et al.). International Council of Explora-
tion of the Sea (ICES) workshop on.the problems of monitoring biological
effects of pollution in the sea. Rapp. P.-V. Reun. Cons. Inst. Explor. Mer
179, 174-181. 1,980.

15. Understanding marine ecosystems in the Gulf of Mexico. UNESCO's Man
and the Biosphere Publication Series, U. S. State Department, Report No. 2,
1-8. 1980.

16. The Apalachicola Experiment: Research and management. Oceanus 23,
14-21. 1980.

17. Acid rain over Florida. Geojourney 1(2), 10-11. 1980.

18. Application of scientific data tq resource management problems in coastal
systems (in press). Soviet-American Ecology Symposium (La Jolla).

19. Between the Idea and Reality. V.P.I. Publ. Prog. Ser. (invited
paper), 31-59.

20. Long-term biological variability and stress in coastal systems. 1982.
Second U. S./U. S. S. R. Symposium; Biological Aspects of Pollutant
Effects on Marine Organisms. Terskol, U. S. S. R.

21. Livingston, R. J., and S. H. Wolfe (1988). Restoration and preservation
ranks of water bodies within the Northwest Florida Water Management
District. Report for the Northwest Florida Water Management District.

22. Prasad, A. K. S. K. 1988. Altas of the klicroflora of North Florida
Rivers. Report for the Florida Department of Environmental Regulation.

23. Livingston, R. J. The Oklawaha River System: Environmental Overview.
Report for the Florida Defenders of the Environment.

Books (Editor or co-editor)

1. Synergistic Bioassays, in Marine Bioassays. Marine Technology
Society, with Geraldine Cox (1974).

2. Proceedings of the Conference on the Apalachicola Drainage System.
Florida Marine Research Publications (1977).

3. Biological Data in Water Pollution Assessment: Quantitative and Statistical
Analyses: American Society for Testing and Materials, with John Cairns,
Jr., and K. Dickson (1978).

4. Ecological Processes in Coastal and Marine Systems. Plenum Press
(1979).

5. The Rivers of Florida (in press, being prepared for publication).

Professional Societies

AIBS, AAAS, American Fisheries Society, American Society of Ichthyologists
and Herpetologists, American Society of Limnology and Oceanography,
American Institute of Fisheries Research Biologists (invited), Gulf
Estuarine Research Society, Ecological Society of America.

Papers Given at Scientific Meetings

"Circadian Respiration Rhythms of Cardinal Fishes" (ASIH, 1970)
Chairman, Pesticide Section (Soc. Lim. Ocean., 1972)
"The Effects of Dredging and Eutrophication on Mulat-Mulatto Bayou
(Escambia
Bay, Pensacola', Florida)" (ASIH, 1973)
"The Impact of the Pesticide Mirex on Aquatic Ecosystems" (1 Oth Annual

Pesticide Residue Conference, 1973)
"The Impact of Pulp Mill Effluents on Fishes of Apalachee Bay" (Virginia
Institute of Marine Science, 1973)
"The Impact of Pulp Mill Effluents on the Aquatic Biota of Apalachee Bay,
Florida" (American Fisheries Society, Annual Meeting, 1973)
with Kenneth L. Heck, Theresa A. Hooks and Michael S. Zimmerman.
"Storm Water Runoff in Estuaries" (Gulf Estuarine Research Society; Ocean
Springs, Mississippi, October, 1974)
"Resource Management and Estuarine Function with Application to the
Apalachicola Drainage System (North Florida, U.S.A.)" (Invited paper,
E.P.A. Conference on Estuarine Pollution Control, February, 1975,
Pensacola, Florida)
"Diurnal and Seasonal Fluctuations of Estuarine Organisms in a North
Florida Estuary: Sampling Strategy, Community Structure, and Species
Diversity" (ASIH, 1975),
"The Impact of Pulp Mill Effluents on Estuarine Plant and Fish Assemblages"
(Invited paper, Phildelphia Academy of Sciences; March, 1975)

"Methods of Sampling Estuarine Systems to Determine the Long-Term
Impact
of Pollutants on Populations and Communities" (invited paper, U.S.
Department of Interior, Fish and Wildlife Service, Washington, D.C.,
April, 1975)
"Avoidance Responses of Estuarine Organisms to Storm Water Runoff and
pulp Mill Effluents" (invited paper, the Third International Estuarine
Research Federation Conference, Galveston, Texas, October, 1975)
"Time as a Factor in Environmental Sampling Programs: Diurnal and
Seasonal Fluctuations of Estuarine and Coastal Populations and
Communities (invited paper, Symposium on the Biological Monitoring of
Water ecosystems, Ed. J. Cairns, Jr., et al., Blacksburg, Virginia, Nov.,
1975)
"The Impact of Pesticides on an Estuarine System" (invited paper, Old
Dominion University; Norfolk, Virginia, February, 1976)
"Environmental Status, of the Apalachicola Bay System" (Florida Defenders
of the Environment, Annual meeting; Gainesville, April, 1976)
"Impact of Organochlorine Compounds on an Estuarine System" (North
Carolina State Univ. Dept. of Zoology,,July, 1976)
"Organochlorine Compounds and. Long-term Changes of Estuarine Fish
Populations in the Apalachicola Bay System" (Invited paper, U.S.
Environmental Protection Agency officials and visiting scientist from
Russia, September, 1976)
"The Apalachicola Drainage System" (Invited paper, the Conservation
Foundation, Joint.Meeting of State and Federal agencies. January,
1977)
"Applications of Scientific Data to Architectural Design in Coastal
Systems" (Invited paper, School of Architecture, Florida A & M
University)
"National Stake in'the Apalachicola River" (invited paper, The
Conservation Foundation, March, 1977)

"The Apalachicola Bay System" (Invited Talk, Coastal Zone Management
Advisory committee, NOAA)
"The Apalachicola Dra]nage System: Functional Interrelationships"
(Invited paper, Annual Meeting; Florida Defenders of the Environment,
March, 1977)
"Impact of Development on Wetlands: Case Study, the Apalachicola
System"
(invited paper, National Wetland Protection Symposium, Environmental
Law Institute and the Fish and Wildlife Service, U.S. Department of the
Interior, June, 1977)
"Statistical Methods Applied to a Four-Year Multivariate Study of a Florida
Estuarine System" (with Duane A. Meeter) (invited paper, American
Society for Testing and Materials; John Cairns, Jr., Ed., June, 1977)
"Temporal Variation of an Estuarine Fish Community" (American Society of
Ichthyologists and Herpetologists, June, 1977), Chairman, Session on
Impact of Pollutants on Fishes.
"The Estuarine Environment" (Invited paper, Symposium on the Coastal
Zone,
University of West Florida; Pensacola, 17-18 June, 1977)
"Estuarine Ecology, Impact of'Forest Management" (CFM Symposium, Flor.
Department of Agriculture and Consumer Services; Gainesville, 17-18
August, 1977)
"Effects of Forest Management Practices on Bay Habitat and Water Ouality"
(invited paper, Apalachicola Planning and Management Program, Florida
Division of Planning, Florida Division of Forestry; Bristol, 31
August, 1977)
."Forestry Activities and the Impact on Apalachicola Bay" (Invited paper,
Coastal Plains Interstate Advisory Board, Wakulla Springs, 14
September, 1977)
"Multiple Factor Interactions: Experimental Design and Field Implications"
(invited paper, Symposium on Pollution and Physiology of Marine
Organisms. Belle W. Baruch Institute for Marine Biology, South
Carolina, 14 November, 1977)
"Summary of Research Objectives" (EPA Ecological Advisory Committee,
Corvallis, Oregon, 3 December, 1977).
Plenary Address: "Coastal Ecosystems." Coastal Zone '78, Symposium on
Aspects of Coastal Zone Planning and Management, San Francisco (14
March, 1978)
Long-term Trends in the Recovery of Florida Coastal Ecosystems Affected by
Pulp Mill Effluents" (Invited paper, American Fisheries Society,
Annual Meeting; Kingston,)
"Temporal Variation and Impact Analysis in Coastal Systems" (Conference
on Ecological Processes in Coastal and Marine Systems, Tallahassee,
Florida) .
The role of Barrier Island in the Productivity and Diversity of Lagoon
Communities in Florida" (invited paper, A. 1. B. S.- Ecological Society of
America, Annual Meeting; Athens, Georgia, August, 1978)
"Long-term Changes in Coastal Systems" (Invited paper, Joint Workshop on
American-Soviet Marine Research. U. S. E. P. A.; Gulf Breeze,

Florida, September, 1978)
"The Apalachicola Bay Ecosystem'." Invited paper, Conservation Foundation
(Washington, D. C.), Tallahassee, Florida (October, 1978)
"Wetlands Food Chains." Invited paper, National Symposium on Wetlands.
14th Annual American Water Resources Conference. Lake Buena Vista,
Florida (November, 1978)
"Long-term Trends in Coastal Ecosystems." Environmental Engineering
Sciences, University of Florida (March, 1979)
"Systems Approaches to Ecological Problems." Invited paper, Australian
Institute of Marine Science; Townsville, Australia (April, 1979)
"Long-term (supra-annual) variability in coastal system--background noise
and environmental stress." Invited paper,'Marine Ecosystems Analysis
Symposium on Ecological Effects of Environmental Stress. Estuarine
Research Federation and New York Sea Grant Institute, New York (June,
1979).
"Short-term Cycles and Long-term Trends in Two North Florida Coastal
Systems." Invited paper, American-Soviet Symposium on Marine Ecol.
Yalta, Russia (July, 1979)
"Spatial/temporal Variability and Long-term Coastal Research in the N. E.
Gulf of Mexico." Man and the Biosphere. Program, U. S. State
Department.
"Design and Conduct of Research Programs for Marine Environment
Management" (Coral Reef Workshop/Great Barrier Reef Marine Park
Authority; Townsville, Australia, August, 1979)
"Trophic Interactions of Coastal Fishes." Invited paper, International
Research Conference (ERF, Biennial Meeting, October, 1979)
"Scientific Research in Estuarine Sanctuaries." Invited paper,
International Estuarine Research Conference (ERF, Biennial Meeting).
Jekyll Island, Georgia (October, 1979)
'Ecosystern Research in the N. E. Gulf of Mexico." Coastal Ecosystem
Research Workshop, National Sea Grant Program; Baton Rouge, LA
(November, 1979)
"The Apalachicola River and Bay Estuarine Sanctuary." Banquet speaker,
18th Annual Southeast Regional ACM Conference; Tallahassee, Florida
(March, 1980)
"Application of Scientific Data to Resource Management Problems in Coastal
Systems." Soviet-American Ecology Symposium, La Jolla (September,
1980)
"Recent Problems in Aquatic Systems of Florida." F.L.A. Fishery Symposium,
Tampa (September, 1980)
"Hydrological Fluctuations, Dettitus Movement, and Interactions of the
Apalachicola Flood Plain with the Apalachicola Bay System." Panel
chairman, National Symposium on Freshwater Inflow to Estuaries. U. S.
Fish and Wildlife Service (September, 1980)
"The Nature of Disturbance and Biological Variability in Estuarine Systems."
Key-note Talk, Gulf Estuarine Research Society Symposium; Pensacola,
Florida (October, 1980) . I
"Man's Impact on.the Distribution and Abundance of Sciaenid Fishes."
Invited paper, Sixth Annual Marine Recreation Fisheries Symposium;

Houston, Texas (April, 1981).
"Development of a Regional Management Strategy for the Apalachicola
Resource." Keynote talk, Regional Planning Council Annual Meeting,,
Blountstown (February 1981).
"Managing Aquatic Resources: Can Science Help." Invited talk, 1 -day semi-
nar. Virginia Polytechnic Institute and State University; Blacksburg,
Virginia (April, 1981).
"The Validation Concept." Invited talk to heads of O.R.D. (E.P.A.)
Laboratories (Corvallis, Athens, Duluth, Gulf Breeze, Naragansett),
Gulf Breeze, Florida (May, 1981).
"Effects of Predation on Benthic Infauna." With Bruce Mahoney. ASZ,
Dallas (December, 1981).
"Long-term Studies in Coastal Ecosystems." National Park Service Work-
shop on the Florida Everglades, Miami, Florida (January, 1982)..
"Seasonal Fluctuations of Benthic Infauna: Predation." With Bruce
Mahoney. Benthic Ecology Meeting, Harvard (March, 1982).
"The Application of Research to Long-term Planning and Management of the
Tri-River System." Technical Workshop, Floodplain Processes in
Nutrient Transport. U. S. Geological Survey (April, 1982).
"Research Design in the Estimation of Natural Variability and Stress in
Aquatic Systems." Workshop on "Meaningful Measures of Marine
Pollution Effects"; N.O.A.A., E.P.A., Pensacola (April, 1982).
"Floodplains and Wetlands--Values and Hazards of Natural Systems." Col,
of Law Symposium on "Local Options for Floodplains and Wetlands
Man agement." University of Florida, Gainesville (September 1982).
"Apalachicola River/Bay Interactions." Apalachicola Oyster Industry
Conference, Apalachicola (October, 1982).
"Application of Research to Resource Management: Case History, the
Apalachicola Estuary." Plenary Speaker, International Symposium on
Utilization of Coastal Ecosystems. Rio Grande, Brazil (November, 1982).
"Tropic Organization of a Seagrass Fish Association." Invited Paper.
Oregon State University, Newport, Oregon (April, 1983).
"Verification of Laboratory Results in the Field." Symposium on the
Use of Multispecies Test Systems. Blackburg, Virginia (May, 1983).
"Trophic Organization of Seagrass Fishes." Annual Meeting,
Association of Ichthyologists and Herpetologists. Tallahassee,
Florida (June, 1983).
"The Apalachicola Experiment." Banquet Speaker (invited). Annual
meeting, Association of lchthyologists and Herpetologists.
Tallahassee, Florida (June, 1983).
"Wetland Values of the Apalachicola Drainage." Symposium on Florida's
Wetlands: Florida House of Representatives. Tallahassee,
Florida (August, 1983).
"Long-term Monitoring in Coastal Systems: Research Needs and
Applications." Banquet Speaker (Invited), Workshop on Monitoring
Considerations in the Siting and Operation of Hazardous Waste
Disposal Facilities. Tallahassee, Florida (October, 1983).
"Coastal Seagrass Meadows:'Form and Function." Invited Paper, 7th
Biennial International Research Conference, Estuarine Research

Federation. Virginia Beach, Virginia (October, 1983).
"Field and Experimental Work in Coastal Seagrass Systems." Oregon State
University Marine Science Center, Newport, Oregon (November, 1983).
"Research and Resource Management." Corporate Weekend, Florida State
University Foundation. Tallahassee, Florida (November, 1983).
Florida's Last Natural Waterway: Can Research and Conservation Rescue
It?" Invited Paper, Royal Canadian Institute. Ontario, Canada
(December, 1983).
Trophic Response and Community Structure of Macroi nve rteb rates and
Fishes in a Coastal Seagrass System. Invited Paper, Department
of Zoo]'ogy, University of Texas. Austin, Texas (January, 1984).
"Apalachicola River Basin: An Applied Study," Invited paper. 7th
Annual Applied Geography conference. Tallahassee, Florida
(November, 1984).
"Effects of Barrier Island Development on Associated Lagoon Systems."
Invited Paper, Conference on the Management of Developed
Barriers. National Science Foundation. Virginia Beach, Virginia
(January, 1985).
"Spatial-temporal Changes in Control of Benthic Communities."
Chairman, Session I on Predation/Herbivory. Benthic Ecology
Meeting. Columbia, South Carolina (March, 1985).
"Field Verification of Toxic Waste Impact on Multispecies Microcosms
of Stream Macroinvertebrates." Invited paper, Ninth Symposium:
Aquatic Toxicology and Environmental Fate. A.S.T.M.,
Philadelphia, Pennsylvania (April, 1985).
"Ecosystem Studies in the Gulf of Mexico." Cary Arboretum, New York
(April, 1985).
"Research Perspectives in Wetland Systems." National Wetland Assessment
Symposium. Portland, Maine (June, 1985). -
."Periodic Hypoxic Conditions in the Apalachicola Estuary." Invited
paper. Estuarine Research Federation Conference. Durham, New
Hampshire (July, 1985).
"Scaling Factors in Estuarine Systems--A Thirteen-year Perspective."
Invited paper. Estuarine Research Federation Conference.
Durham, New Hampshire (July, 1985).
"Human Impacts on Tropical and Subtropical Seagrasses of the Southeast.
U.S. Botanical Society of America. Gainesville, Florida (August, 1985).
"Analysis of Apalachicola Oyster Beds." Apalachicola River and Bay
Estuarine Sanctuary Meeting. Apalachicola, Florida (October,
1985).
"Planning and Estuarine Research." Invited participant, North Carolina
Coastal and Estuarine Preplanning Meeting. Duke Marine Laboratory,
Beaufort, N.C. (January, 1986).
"Scaling and Interpretation of Laboratory Field Tests," "Field
Verification of Multispecies Microcosms Using Marine
Macroinvertebrates." 1 Oth Annual Meeting, American Society for
Testing and Materials. Session Chairman: "Laboratory and Field
Comparisons." New Orleans (May, 1986).
"Relationship of Laboratory Results and Field Responses of Estuarine

Assemblages to Toxic Agents." invited paper, Gordon Research
Conference on Estuarine Processes. Plymouth, N.H. (June, 1986).
"The Choctawhatchee River/Bay System." Invited paper, American Water
Resources Association. Wakulla Spring, Florida (April, 1986)
"Ecological Processes of Recruitment in Coastal Epibenthic Macrobiota:
A Comparative Approach." Invited paper, International Conference
on Recruitment in Demersal Communities. Ciudad del Carmen, Mexico
(April, 1986).
"Use of Macroinvertebrate Microcosms in the Evaluation of Toxic Waste
Sites." Invited paper, ASTM meeting. Bal Harbour, Florida
(November, 1986).
"Algal Microcosms in Toxic Waste Studies: Field Verification of
Laboratory Results." "Use of Research in the Management of the
Apalachicola Drainage System." Invited papers, Symposium on."Algae
in Freshwater Systems." Madras, India (January, 1987). -. .
"Inadequacy of the Use of Species-level Designations in Ecological
Studies." Invited paper, Sixth Biennial Conference on Ecological
and Evolutionary Ethology of Fishes. Lamar University, Beaumont,
Texas (17-20 May, 1987).
"Ecosystem Research and Resource Management." Keynote address
(invited), Florida Bay Symposium. Miami, Florida (31 May-5 June,
1987).
"Conference on the Rivers of Florida." Conference coordinator.
"Apalachicola River System"; "Choctawhatchee River System" (9-10
June,1987).
"Ecosystem Research in the Open Ocean." Invited paper, panel member.
Seventh International Ocean Disposal Symposium. Nova Scotia,
Canada (21-25 September, 1987).
"Recruiting Researchers." Invited paper, National Estuarine Research
Reserve Workshop. Apalachicola, Florida (19 October, 1987).
"Field Verification of Estuarine Macroinvertebrate Microcosms: The Use
of Trophic Organization and Guilds for Predicting Toxic Impact."
Invited paper. "Case Study of Application of Scie'nce to
Management: The Apalachicola River-Bay System." Invited paper.
"Interannual Variability of Biological Processes in Estuarine
Systems: Trophic Units and Guilds." Invited paper. Ninth
Biennial International Estuarine Research Conference. Estuarine
Research Federation, New Orleans, Louisiana (25-27 October, 1987).
"Impact of Climate Change on Yields of Estuarine Fisheries." Invited
paper, North American Conference on'Prepariing for Climate Change.
Washington, D.C. (27-29 October, 1987).
"The Oklawaha: An Ecological Point of View." Invited paper, Florida
Defenders of the Environment, Marion County, Florida (31 October,
1987).
"Environmental Research: How Much is Enough?" Plenary address,
invited, Eighth Annual Minerals Management Service, Gulf of Mexico
OCS Region. New Orleans, Louisiana (1 -3 December, 1987).
The Apalachicola Problem" Big Bend Sierra Club (18 April, 1988)
"Ecological linkages: forests, rivers, and estuaries" Florida Audubon Society

Annual Meeting. (27 October, 1988)
"The Lake Jackson ecological situation." Council of Neighborhood
Associations, Leon County. (14 November, 1988)
"Lake J-ackson ecology" Florida Wildlife Federation. (24 January, 1989)
Lake Jackson: Microcosm of Florida's Environmental dilemma." Florida
Alumnae Association dinner. (January, 1989)
"The ecology of Florida's estuarine systems: dark days ahead." Organization
of Artificial Reefs. (9 March, 1989).

Reviewer of Manuscripts and Proposals:

National Institutes of Health National Science Foundation (Popula-
U. S. Environmental Protection Agency tion Biology and Physiological
National Sea Grant Program (NOAA) Ecology; Environmental.Biology)
National Water Quality Commission Virginia Journal of Science
Florida Scientist Ecology
Biogeography Ecological Monographs
Transactions of the American Illinois Natural History Survey
Fisheries Society Harper & Row, Publishers, Inc.
Science Virginia Polytechnic Institute and
Estuarine and Coastal Marine Science State University (review of
Northeast Gulf Science faculty member)
Estuaries American. Society for Testing and
Canadian J. of Fisheries and Materials
Aquatic Sciences Florida Department of Environmental
Contributions in Marine Science Regulation
J. Experimental Marine Biology and National Geographic Society
Ecology American Fisheries Society (book)
Marine Biology Hydrobiologia
Copeia American Institutute of Biological
Bulletin of Marine Science Sciences (book)
Fishery Bulletin Springer-Verlag
Archives of Environmental Contamina- Estuarine Research Federation
tion and Toxicology Hudson River Foundation

Teaching and Graduate Students

Courses taught at Florida State University

Bio. 105 (General Biology), Bio. 201 (Fundamentals of Biology),
Bio. 203 (Fundamentals of Ecology), Bio. 426 (Aquatic Pollution
Biology), Bio. 501, (Comparative Physiology), Bio. 540 (Physiological
Ecology of Fishes), Bio. 541 (Tropho-dynamics of Aquatic Systems), Bio. 646
(Advanced Ichthyology), Bio. 655 (Vertebrate Seminar), ZOO 4454C (Biology
of Fishes), ISC 2937-01 (Natural Science Honors. Seminar).Madne Biology

Graduate Students:

Graduated:

1. Columbus H. Brown, M.S. (The effect of photoperiodism on the
respiration of the channel catfish) - presentlyemployed as a biologist
with the U. S. Fish and Wildlife Service. 1973.
2. Stephen Brice, M.S. (The effects of methyl mercury on the channel cat-
fish Ictalurus punctatus) - presently employed as a research biologist
with Dow Chemical Corporation. 1973.
3. Theresa Ann Hooks, M.S. (An analysis and comparison of the benthic
invertebrate communities in the Fenholloway and Econfina estuaries of
Apalachee Bay, Florida) - graduate of (environmental) law at F. S. U.
Law School. 1973. 1 -
4. Bruce D. DeGrove, M.S. (The effects of mirex on temperature selection
in the sailfin molly, Poecilia latipinna) - presently employed as a
biologist with the Trustees of the Internal Improvement (State of
Florida). 1973.
5. Kenneth L. Heck, Jr., M.S. (The impact of pulp mill effluents on spe-
cies assemblages of Opibenthic marine invertebrates in Apalachee Bay,
Florida). 1973
6. Gerard G. Kobylinski, M.S. (Translocation of mirex from sediments and
its accumulation by the hogchoker (Trinectes maculatus)). 1974.
7. Frank G. Lewis, M.S. (Avoidance reactions of two species of marine
fishes to kraft pulp mill effluents). 1974.
8. Aureal J. Tolman, M.S. (Effects of mirex on the ac-
tivity rhythms of the diamond killifish, Adinia xenica). 1974.
9. Claude R. Cripe, M.S. (The effects of mirex on a simulated marsh
system). 1974.
10. Michael Zimmerman, M.S. (A comparison of the benthic macrophytes of
polluted system (Fenholloway River) and an unpolluted system (Econfina)
in Apalachee Bay, Florida). 1974.
11. Paul Muessig, M.S. (The determination of pathways of mercury con-
centration and conversion within specific organs of channel catfish
(Ictalurus punctatus)). 1974.
12. Christopher C. Koenig, Ph.D. (The synergistic effects of mirex and DDT
on the embryological development of the diamond killifish; Adinia
xenica) - currently asst. professor, College of Charleston. 1975.
13. Susan Drake, M.S. (The effects of mercury on the development of the
zebrafish). Fall quarter, 1975.
14. Allan W. Stoner, M.S. (Growth and food conversion efficiency of pin-
fish (Lagodon rhomboides) exposed to sublethal concentrations of
bleached kraft mill effluents). Winter quarter, 1976.
15. Roger A. Laughlin, M.S. (Avoidance of blue crabs (Callinectes sapidus)
to storm water runoff). Spring quarter, 1976.
16. George Gardner, M.S. (Behavioral reactions of pinfish to pulp mill

effluents). Summer quarter, 1976.
17. Peter Sugarman, M.S. (Effects of bleached kraft mill effluents on
activity rhythms of the pinfish, (Lagodon rhomboides)). Spring
quarter, 1977.
18. Bruce Purcell, M.S. (Effects of storm water runoff on grass bed com-
munities in East Bay). Spring quarter, 1977.
19. James Duncan, M.S. (Short-term impact of clearcutting activities on
epibenthic fishes and invertebrates in the Apalachicola Bay system).
Spring quarter, 1977.
20. Peter Sheridan, Ph.D. (Trophic relationships of fishes in the
Apalachicola Bay system) - presently Marine Ecologist, Bears Bluff
Laboratory, U. S. EPA. Spring quarter, 1978.
21. Allan Stoner, Ph.D. (Ecological relationships and feeding response of
the pinfish, Lagodon rhomboides). Summer quarter, 1979.
22. Steven Osborn, M.S. (Ecological relationships of ophiuroids in
Charlotte Harbor). Fall quarter, 1979.
23. Joseph Ryan, M.S. (Day-night feeding relationships.of grassbed
fishes). Spring quarter, 1981.
24. Holly Greening, M.S. (Spatial/temporal distribution of invertebrates
in grassbeds of Apalachee Bay). Summer quarter, 1980.
25. Bruce MacFarlane, Ph.D. (Effects of variations in pH on topminnow phy-
siology and behavior). Spring quarter,. 1980.
26. Pat Dugan, M.S. (Long-term population changes of epibenthic macro-
invertebrates in Apalachee Bay, Florida). Summer Quarter, 1980.
27. Brad McLane,, M.S. (impact of stormwater runoff on benthic
macroi rive rteb rates). Fall Quarter, 1980.
28. Kathy Brady, M.S. (Larval fish distribution in Apalachee Bay).
29. Duncan Cairns, M.S. (Detritial processing in a subtropical southeastern
' drainage system) Fall Semester, 1981.
30. Bruce Mahoney, Ph.D. (The role of predation in seasonal fluctuations
of estuarine communities). Summer, 1982.
31. Will Clements, M.S. (Feeding Ecology of Filefish in Apalachicola Bay,
. Florida). Summer, 1982.
32. Graham Lewis, Ph.D. (Habitat Complexity in a Subtropical Seagrass
Meadow). Fall, 1982.
33. Ken Leber, Ph.D. (Feeding Ecology of Decapod Crustaceans). Summer,
1983.
34. Kevan Main, Ph.D. (Predator-prey Interactions in Seagrass Beds: The
Response of Tozeuma carolinense). Winter, 1983.
35. Kelly Custer, M.S. (Gut Clearance Rates of Three Prey Species of the
Blue Crab). Summer, 1985.
36. J. Michael Kuperberg, M.S. (Response of the marine macrophyte
Thalassia testudinum to herbivory). Fall, 1986.
37. Susan Mattson, M.S. (The effect of post-settlement predation on com-
munity structure of epifauna associated with cockle shells). Fall,
1986.
38. Joseph L. Luczkovich, Ph.D., (The patterns and mechanisms of selec-
tive feeding on seagrass-meadow epifauna by juvenile pinfish,
Lagodon rhomboides). Fall, 1987.

39. Jon A. Schmidt, Ph.D. (Patterns of seagrass infaunal polychaete
recruitment: influence of adults and larval settling behavior).
Fall, 1987.
40. David Bone, Ph.D. (Response of seagrass invertebrates to toxic
agents). Fall, 1987.
41. Carrie Phillips, M.S. (Influence of physical disturbance on
infaunal macroinvertebrates: seagrass beds vs. unvegetated areas).
Spring, 1987.
42. Frank Jordan, M.S. (Trophic organization of fishes in the Choctawhatchee
River.) Spring, 1989.

Current

Jeff Holmquist (Ph.D.)
Jutta Schmidt-Gengenbach (M.S.)

Public SerVice
r
State (* =active)
Interstate 1-0 Environmental Study Team (1970), Florida Department of
transportatiom
Chairman, Select Study Committee on Mirex, Governors Natural Resources
Committee.
Advisor to Department of Transportation on Dredging and Filling Activities.
Advisor to Attorney General's Office on pollution issues.
Member, Interinstitutional Technical Advisory Committee on Environmental
Affairs for Florida Pollution Control Department.
Advisor to numerous House and Senate Committees on Environmental
Affairs.
Advisor to Department of Natural Resources on determination of land
acquisition under the environmentally endangered lands program.
Advisor to Leon County School System for environmental education in north
Florida.
Testimony before State Cabinet on environmental affairs.
Provided scientific data that went into determination of the Florida
Cabinet's decision to reject a dam to be built on the Apalachicola
River by the U. S. Army Corp of Engineers.
Advisor to the Calhoun County Board of Commissioners concerning
environmental issues associated with the Apalachicola Bay system.
Environmental consultant on DRI for SW Florida Regional Planning Council.
Program Chairman and Speaker, Florida Defenders of the Environment
Annual Meeting (1976): Controversial Waterways with Emphasis on the
Apalachicola Drainage System.
Florida Defenders of the Environment Annual Meeting (1977): Three
Florida Rivers.
Advisor, Florida Department of,Envi ron mental Regulation, Florida Dept.
of Natural Resources, Florida Game and Fresh Water Fish Commission,
Florida Division of State Planning (Department of Administration)

regarding the application of scientific data for a comprehensive manage-
ment program for the Apalachicola Valley.
Reviewer (at the request of the Franklin County Board of County
Commissioners) of DRI associated with development of St. George
Island (1977).
Reviewer for various state agencies of reports concerning environmental
impact studies (e.g., the "Chesher Report" concerning the effects of
canals and development on water quality in the Florida Keys).
Trustee, Florida Defenders of the Environment. Provide scientific infor-
mation for environmental problems.
Member, Citizen's Advisory Committee on Coastal Zone Management for the
Apalachee Regional Planning Council.
Participant (at request of the Honorable Ralph Turlington, Commissioner of
Education), Environmental Education Activities in the Apalachicola
River and Bay Resource Management and Planning Program.
Scientific advisor (unpaid), Franklin County Board of County Commissioners,
1972-present.
Scientific advisor (unpaid), Wakulla County Board of Commissioners,
1980-present.
Member, Science Advisory Board, Florida League of Anglers.
Member, Shellfish Sanitation Task Force, Florida Department of Natural
Resources.
Advisor (unpaid),.Franklin County School Board. Development of
environmental science in secondary schools.
Advisor (unpaid), Wakulla County Commercial Fisherman's Association.
Advisor (unpaid), Concerned Citizens Association of Wakulla County.
Advisor, Apalachee Regional Planning Council
Member, Board of Directors, Environmental Service Center (Florida
Defenders of the Environment)
Member, Science Advisors Committee (Review of the Flint River;
Chairperson: Ruth Patrick).
Member, Sanctuary Management Committee (in charge of research and edu-
cation in the Apalachicola River and Bay National Estuarine
Sanctuary).
Scientific advisor to Migrant Workers' Association concerning the use
of the pesticide Temik in Florida
Scientific Advisor to the Florida Department of Environmental
Regulation, the Audubon Society, and Getty Oil Company con-
cerning oil drilling in the Pensacola Bay system
Scientific Advisor to the Apalachee Regional Planning Council and
local citizen's groups concerning heavy metal pollution of the
Chipola River
Member, Health Advisory Council, Florida Department of Health and
Rehabilitative Services
*Member, Dog Island Environmental Advisory Board
Old Pass Lagoon Technical Advisory Committee (NWFWMD)
Bioassay Task Force (FDER)
Member, Apalachicola Bay Area Resource Planning and Management
Committee

Member, Apalachicola Bay Reserve Advisory Committee
Member, Scientific Review Committee, DOI Offshore Environmental Studies
*Member, Basin Advisory Committee, Northwest Florida Water Management
District
*Member, Technical Advisory Group, Suwannee River Water Management
District
*Member, Perdido Bay Cooperative Management Project.
Participant, The Florida Water Story, educational film.

Federal active)

Environmental Coordinator for U. S. Environmental Protection Agency.
Coordinator, Estuarine Management Proposal, Florida Sea Grant (1973,
1974).
Advisor to U. S. Senator Lawton Chiles on environmental affairs and
the energy "crisis."
Invited participant in formal presentation to the Reuss Committee on
Conservation and Natural Resources (U. S. House of Representatives).
Advisor to the Select Study Committee on Mirex, Environmental Protection
Agency.
Chairman, STAEP panel on Kepone/mirex/hexachlorocyclopentadiene:
Reviewer
of environmental and health implications for the National Academy of
Sciences (Environmental Studies Board, National Research Council).
Member, Ad-hoc group to review the 1975 Water Research Strategy Doc of
the Environmental Protection Agency. This included a review of
research carded out by the E.P.A.
Participant in U. S. Environmental Protection Agency Conference and re ,port
(presented to the Congress of the United States) concerning Estuarine
Pollution Control.
Special consultant to the National. Commission on Water Quality (N.C.W.Q.)
to determine the economic, social, and environmental impact of
achieving or not achieving the goals of the Federal Water Pollution
Control Act of 1972.
Advisor, Office of Coastal Zone Management (NOAA) concerning the
elegibility of the Apalachicola Bay system for inclusion in the National
Estuarine Sanctuary Program.
Coordinator (with the Conservation Foundation) of a series of meetings
with federal and state agencies concerning the development of a manage-
ment program for the Apalachicola Valley.
Participant in the "Operation Fish Bowl" planning and advisory group for
the U S. Army Corps of Engineers regarding the development of
"Principles and Standards for Planning Water and Related Land
Resources" for the Tri-River (Flint-Chattahoochee-Apalachicola) system.
Participant in the development of a joint effort with the Office of
Monitoring and Technical Support (U. S. Environmental Protection
Agency), the Environmental Monitoring and Support Laboratory (U. S.
Environ 'mental Protection Agency), and the National Aeronautics and

Space Administration (NASA) to apply remote sensing technology to the
monitoring of stress due to upland runoff on the Apalachicola Bay
system.
Member, Ecology Committee, Science Advisory Board, U. S. Environmental
Protection Agency (1978-1982). (Review 5-year plan for environmental
research, advise on "air/water' quality standards, etc.)
Testimony for Congressional Hearing, Barrier Islands National Parks Bill (H.
R. 5981), Washington, DC (March, 1980)
Advisor, Australian Institute of Marine Science and Malcolm Fraser (Prime
Minister of Australia) Research Program for the Great Barrier Reef.
Advisor, Nature Conservancy and Trust for Public Lands, Inc., con-
cerning land purchases in Florida
Advisor to various federal environmental officers concerning environ-
mental problems in Florida
Consultant, Environmental Effects, Transport and Fate Committee, U.S.
Environmental Protection Agency
Member, Extramural Review Board, U.S. Environmental Protection Agency
Member, Habitat and Environmental Advisory Panel, Gulf of Mexico
Fishery Management Council
Vember, Advisory Committee to the Man and the Biosphere Program
(United Nations).
*Member, Board of Scientific Advisors, The Wetlands Fund.
Advisor, Alliance for Chesapeake Bay.

CHCOTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 1

Standard Operating Procedures

(analytical protocols for water quality chemistry)

Robert J. Livingston
Center for Aquatic Research
and Resource Management
Florida State University
Tallahassee, Florida 32306

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 2

Contents
TITLE PAGE

I Physical -Examination ............................................................. 3
1 - Temperature ................................................................ 3
2. Salinity/Conductivity .................................................. 3
3. Dissolved Oxygen ......................................................... 3
4. pH ................................................................................. 3
5. Secchl ...................................... .................. 4
6. Depth ...................................... 4
II. Collection and Preservation of Samples ................i ................ 5
1 . Collection .................................................................... 5
2. Preservation ................................................................ 6
Ill. Physical Characteristics ....................................................... 7
1 - Apparent Color: Spectroscopic Method ........................ 7
2. Turbidity: Nephelometric Method ............................... 7
3. Total Dissolved Solids at 1800C .................................. 7
4. Total Suspended Solids at 103-1050C ........................ 7
5. Fixed and Volatile Solids at 5500C .............................. 8
6. Biochemical Oxygen Demand ....................................... 9
7. Dissolved Oxygen, Azide Modified Winkler ................. 10
8. Chemical Oxygen Demand ............................................. 11
9. Particulate Organic Carbon ......................................... 12
10. Particulate Organic Matter ......................................... 12
11. Total Alkalinity ............................................................ 13
12 " Chlorophylls, a, b, and c ............................................. 14
IV. Nutrients ................................................................................. 16
1. Nitrogen, Semi-micro Kieldahl .................................. 16
2. Nitrogen, Nitrate, Cadmium Reduction ....................... 17
3. Nitrogen, Nitrite ......................................................... 19
4. Ammonia, Ion sensitive electrode ............................... 21
5. Ammonia, Phenate Method .......................................... 22
6. Ammonia, -Nesslerization ............................................ 23
7. Phosphates, Filtration ................................................ 25
8. Phosphates, Condensed ................................................ 25
9. Phosphates, Total ........................................................ 26
10. Ortho- Phosphates, Ascorbic Acid ............................... 26
V. Solutions ................................................................................. 28
1 . Lugals Solution .......................... .................................. 28
2. Bouin's Solution28 ...................................................... 28
3. Probe Juice, Y.S.I.,D.0 ................................................ 28
4. Probe Cleaner, Y.S.I., S.C.T.' ' ................... 28
5. Probe Cleaner, Y.S.I., D.0 ............................................ 28
VI. Instruction Manuals ............. Wi** -- .... -**-- ......- ......... 29
1. YSI Model 33 and 33 -C,T Meters ........................ 29
2. YSI Model 57 Dissolved Oxygen Meter ....................... 30
3. Corning Calomel Electrodes ........................................ 31

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 3

L Physical Examination
(performed in the field)

1. Temperature
Method Number 212, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.
Temperature in degrees Centigrade is measured with the calibrated temperature
probe in the YSI model 57 Oxygen meter. This reading is compared in the field with a
similar reading from the YSI model .33 S-C-T Meter. Temperature readings are taken at
the top and the bottom of the water column on site.

2. Salinity/Conductivity
Method Number 205' Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 198.5.
Percent salinity is measured in the field with a YSI model 33 S-C-T meter
calibrated in the laboratory against Standard Seawater. In waters with no appreciable
salinity, conductivity in gmhos is measured with the same meter. Readings are taken at
the top and bottom of the water column on site.

3. Dissolved Oxygen
Method Number 421, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.
Dissolved oxygen in mg/L is measured in the field with a YSI model 57 Oxygen
Meter calibrated against standards analyzed by the azide modified Winkler technique.
Readings are taken on site at the top and bottom of the water column. The oxygen meter
is air calibrated in the field.

4. pH
Method Number 423, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.
The pH is measured in pH units, the negative logarithm of the Hydrogen ion
concentration, with a Corning 610A pH Meter equipped with a Calomel electrode that is
calibrated in the laboratory. Readings are taken from the top and bottom of the water
column in the field and in the laboratory. The meter is calibrated to pH 4, pH 7, and pH
10 with buffer solution in the field.

CHOCTAWHATCHEE 7 S. 0. P.
Date 12/13/89
Page Number 4

5. Secch!
The Secchi disk is lowered into the water slowly until the
characteristic black and white pattern can no longer be distinguished. This depth is
recorded in meters.

6. Depth
Depth is recorded with a graduated meter cord attached to a lead weight, which is
lowered to the bottom. At contact, depth is recorded in meters.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 5

11. Sample Collection and Preservation of Samples

1. Collection

The result of any test can be no better than
the samples on which it is performed.
An old Axiom

The objective of sampling is to collect a portion of material small enough in
volume to be transported conveniently and handled in the laboratory ..while still
accurately representing the material being sampled. This implies that the relative
proportions or concentrations of all pertinent components will be the same in the
samples as in the material being sampled and that the sample will be handled in such a
way that no significant changes in composition will occur before the tests are made.
Sample bottles must be rinsed with the water being sampled at least three times.
Sample containers that are to be re-used are rinsed at least three times with dl water,
dried, and then sealed to avoid any contamination. If phosphates are to be analyzed, the
use of detergents must be avoided, unless the sample containers are acid washed with
warm 10% HCI.
Samples collected at a particular time and place can represent only the
composition of the source at that time and place. Grab samples are collected with a
Kemmerer sampler at the bottom of the water column. Avoid collecting detritus by
taking the sample a few centimeters above the soil/water interface. Surface samples are
collected by lowering an inverted sample container beneath the water/air interface and
righting it. Avoid collecting any flotsam and jetsam by filling the sample container 5cm
beneath the surface. Avoid entrapping air in the filled sample container. The sample
must be kept on ice in the dark until it is received at the laboratory.
When a source is known to vary with time, samples must be taken with
appropriate frequency to monitor the extent of these variations. In such a situation, the
location and the time of sample collection must be accurately duplicated. In open water,
a Loran can assure site location to within a hundred feet, otherwise landmarks must be
judiciously chosen.
Samples are put on ice in the dark immediately to assure stability of constituents
until they can be analyzed in the lab. Before delivery of the sample to the lab, a chain of
custody form must be filled out detailing the volume of the sample, the location of the
site, the date and time of sampling, the name of the samplers, the project and/or the
parameters to be analyzed, the technique by which the sample was obtained, and the
methods of preservation.
Samples are to be delivered to the lab with all possible haste, it delivery time
exceeds 24 hours, correct preservation techniques must be observed. Generally, a
sample will be accepted by the laboratory if they are on ice, with a proper chain of
custody form. Once received samples are allowed to rise to ambient temperature before
analysis.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 6

2. Preservation
The unequivocal preservation of samples is fundamentally impossible.
Regardless of the preservation technique, complete stability for every constituent can
never be achieved. It is best to analyze samples as soon as possible after collection, and
then to judiciously determine the type of preservation to be utilized.

Measurement Container Preservative Holdin
Color P, G Cool, 40C 48 hours
Conductance P, G Cool, 40C 28 days
pH P, G None None
Filterable Residue P, G Cool, 40C 7 days
Non-filterable Residue P, G Cool, 40C 7 days
Temperature P, G None None
Turbidit P, G Cool, 40C 48 hours
Alkalinity P, G Cool, 40C 14 days
Ammonia P, G Cool, 40C, H2SO4 to pH 28 days
Kjeldahl Nitrogen P, G Cool, 40C, H2SO4 to pH <J! 28 days
Nitrate P, G Cool, 40C 48 hours
Nitrite P, G cool, 40C 48 hours
Oxygen, dissolved P, G None None
Ortho-Phosphate G Cool, 40C, no acid 48 hours
Total Phosphate G Coo I, 40C, H2SO4 to pH < I,c 28 days
Phosphate, T. dissolved G Cool, 40C, H2SO4 to pH <,, 24 hours
DOD P, G Cool, 40C 48 hours
CCD P, G Cool, 40C, H2SO4 to pH <,, 28 days
Organic Carbon P, G 1 Cool, 40C, H2SO4 to pH < 4 28 days

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 7

111. Physical Characteristics
(analyzed in the our Chemistry Laboratory)

1. Apparent Color: Spectroscopic Method
E. P. A. approved HACHTM method, and Method Number 204 B., Standard Methods for
the Examination of Water and Wastewater, Sixteenth Edition, 1985.
Samples are allowed to settle. Decant 25ml from the sample container into the
HACHTM graduated boro-silicate colorimetric vial. The color is measured against a dl
water blank on one of two different colorimeters ( HACHTM DR/1 or HACHTM DR/A
using an alpha-platin um -cobalt filter. Colorimetric values range from zero to 500
units. One color unit is equal to 1mg/L platinum as the chloroplatinate ion.

2. Turbidity: Nephelornetric Method
Method Number 214 A., Standard Methods for the Examination of Water and
Wastewater, Sixteenth Edition, 1985.
Fill the sample tube with sample and standards which have been homogenized,
allowing all air bubbles to escape. The standard blank is turbidity-free water from
HACHTM sealed in ampules measuring 0.61, 10.0. 100.0, and 1000.0 NTU. A HACHTM
model 2100A turbidometer equipped with a tungsten-filament lamp and photoelectric
cells to detect light scattered at 900 to the path of incident light is used. Sample vials
are kept scrupulously clean and scratchless. Between samples, wash the vials with
three volumes of dl water, and zero the instrument. Be sure to dry the surfaces of the
vial, particularly it's base, before placing the sample in the turbidometer. Turbidity
@values range from 0 NTU to 1000 NTU, and roughly approximate the old Jackson Candle
Turbidity units.

3. Total Dissolved Solids at 1800C
Method Number 209 B., Standard Methods for the Examination of Water and
Wastewater, Sixteenth Edition, 1985.
(1) Glass Fiber Filter Disk : Whatman(P 4.25cm dia. 934-AH. Rough side down.
(2) Evaporating Dish ignite at 550 1 500C for one hour in the muffle furnace to rid it
of possible contaminants.
(3) 2.5-200.Omg of sample should be obtained in less than 10 minutes filtering time.
More sample may lead to the entrapment of water in a thick residue.
(4) Filtration : Filter a measured volume of well-mixed sample and wash with three
10ml volumes of di water. Transfer the filtrate to a weighed evaporation dish and heat
in an oven at 180:L20C and cool in a dessicator. Repeat until a const ant weight is
obtained, or until weight loss is less than 4% of the previous weight, or 0.5mg,
whichever is less.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 8

Calculations

mg total dissolved solids/L (A-B) x 1000
sample volume in ml

4. Total Suspended Solids at 103-1050C
Method Number 209 C., Standard Methods for the Examination of Water and
Wastewater, Sixteenth Edition, 1985.
(1) Glass Fiber Filter Disk : Whatman@ 4.25cm dia. 934-AH. Rough side down. Ignite'
at 5500C for 15 minutes to rid the filter of contaminants. Store in a dessicator, and
weigh before use.
(2) Sample: select suitable volume of sample to obtain between 2.5-200mg of sample
in less than 10 minutes filtering time.
(3) Filtration: assemble filtering apparatus and begin suction. Wet
filter, and filter a well-mixed volume of sample. Wash with three 10ml volumes of
distilled water. Remove and dry filter in an oven for at least 1 hour at 103-105C. Cool
the filter in a dessicator. Repeat cycle until weight is constant, or weight loss is less
than 4% of previous weight, or weight loss is less than 0.5mg, whichever is less.

C_glculations

mg total suspended solids/L (A - B) x. 1000
sample vol.(ml)
where A =.weight of filter + dried residue *(mg), and
B = weight of filter (mg).

5. Fixed and Volatile solids at 5500C
Method Number 209 D., Standard Methods for the Examination of Water and
Wastewater, Sixteenth Edition, 1985.
(1) Sample: Oven dried residue from the Total Dissolved Solids and the Total Suspended
Solids tests. These two residues must be worked up separately, thus there will be two
different fixed and volatile determinations.
(2) Muffle Furnace:. Ignite the sample at 550 :L 500C for at least an hour in a muffle
furnace. Cool in dessicator and repeat cycle if weight loss is non-existent, less than 4%
of previous weight, or less than 0.5mg.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 9

Calculations
mg volatile solids/L (A - x 1000
sample volume (ml)

mg fixed solids/L (B - Q x 1000
sample volume (ml)

A = weight of dried residue + dish + filter before ignition (mg)
B = weight of dried residue + dish + filter after ignition (mg@
C = weight of dish + filter (mg)

6. Biochemical Oxygen Demand
Method Number 507, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.
This empirical bioassay measures the dissolved oxygen consumed by microbial life
assimilating and oxidizing the organic matter present. 300, 275, 200, and 125ml of
the sample are incubated for five days in the dark, at 200C, in standard BOD bottles.
The remaining portion of the BOD bottle is filled with a HACHTM BOD nutrient solution.
The reduction in dissolved oxygen concentration during the incubation period yields a
measure of the biochemical oxygen demand. Reagent, nutrient, dl Water and glucose/
glutamic acid blanks are run simultaneously, to make sure that there is no
contamination from other sources. Determination of dissolved oxygen can be
accomplished with either the azide modified Winkler technique, or with a YSI dissolved
oxygen meter and BOD bottle probe equipped with a stirrer boot.
Run checks assuring that contamination is not affecting the BOD. The glucose-
glutamic acid standard check is one of the best. Dry reagent-grade glucose and reagent-
grade glutamic acid at 1030 for one hour. Take 150 mg of each and dilute to one liter.
This solution must be prepared fresh immediately before use. If the 5d 200C BOD value
of the glucose-glutamic acid standard check (use a 2% dilution) is less than 200 ;L
37mg/L, reject any BOD determinations. Run a nutrient blank and a dl water blank as
additional checks.

Calculations

BOD, mg/L @D
P
D, ='DO of diluted sample immediately after preparation, mg/L.
D2 = DO of diluted sample after 5d incubation at 200C, mg/L.
P = decimal volumetric fraction of sample used.

Standard Deviation 0.120mg/L

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 10

7. -Dissolved Oxygen: Azide Modified Winkler
Method Number 421 B, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, . 1985.

Reaaents

(1) Manganous Sulfate Solution: 364g MnS04 H20 in distilled water, filter and dilute
to 1 L.
(2) Alkali- iodide- azide reagent: 5OOg NaOH (or 700g KOH) and135g Nal (or 150g
KI) in distilled water, dilute to 1L. Add 10g NaN3 dissolved in 40ml distilled water.
Should not give color with starch solution when diluted or acidified.
(3) Sulfuric Acid: concentrated.
(4) Starch: 2g laboratory-grade soluble starch and 0.2g salicylic
acid in 100ml distilled water.
(5) Standard Sodium Thiosulfate titrant: 6.205g Na2S203 5H20 in distilled water.
Add 1.5ml 6N NaOH or 0.4g of solid NaOH and dilute to 1000ml. Standardize with bi-
iodate solution.
(6) Standard Potassium bi-iodate solution: 812.4mg KH(103)2 inIO00ml di water.
To standardize, dissolve 2g KI in 100-150mi water. Add 1ml 6N H2S04 and 20ml of
standard bi-iodate solution. Dilute to 200ml, and titrate liberated iodine with
thiosulfate titrate to a pale straw color. Add starch, and continue titrating until blue
color disappears.
(7) Potassium Fluoride Solution: 24.689g of anhydrous KF in 100ml
H20.

Procedure

(1) To sample add 1ml MnS04 solution.
(2) Add I ml alkali-iodide-azide reagent.
(3) Stopper to exclude air bubbles and mix by inverting bottle.
(4) After ppt settles to about 1/2 volume of bottle, leaving a clear supernate, add 1 ml
conc. H2SO4. Restopper and mix.

Calculations

(1) For titration of a 200ml sample, 1ml 0.0021 M NaS203 = 1mg DO/L
(2) To express results in percent saturation at 1 atm pressure (101.3 kPa.), use
solubility data in the table on the next page. Warning: Brown-colored waters containing
tannic acid and humic acids interfere with the Winkler test; on such waters a D.O. meter
must be used.
Standard Deviation 20gg/L

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 11

8.,Chlemical Oxygen Demand, Closed Reflux, Colorimetric
Meth6d NU46i 508 C, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Editioin, 1985.

ReagentsO
(1) Digestion Solution : 10.216g K2Cr2O7 ( dried at 103C for 2 hours ) in 500ml dl
water. Add 167ml concentrated H2SO4 slowly with stirring, and then add 33.3g HgS04.
Let all the-components dissolve, cool to room temperature, and then dilute to 1000ml.
(2) .8i!verISUIfU?I,c Acid Solution : Add A92SO4 crystals or powder to concentrated
H2S04, at a rate of 5.5g AgS04/kg H2SO4 (5.5g/544.8ml). Let it stand for 1 to 2 days
to dissolve the Ag2SO4.
(3) Potassium Hydrogen Phthalate ( KHP standard : Lightly crush and dry the KHP to
constant weight at 1200C. Dissolve 425mg Iin di water and dilute to 1000ml. Stable
when refrigerated for up to 3 month in the absence of any visible biological growth.

Procedure

(1) Homogenize sample at high speed for 2 minutes. This insures a uniform
distribution of suspended solids, and thus improves the accuracy and reproducibility of
test results.
(2) Prepare reaction vials in the optical grade screw-cap vials.
Silver/Sulfuric Acid Reagent .............. 3.5ml
Digestion Solution .................................... 1.5ml
Sample Size ................................................. 2.5ml
(3) Holding the vial by the cap in an empty sink, swirl the vial using a circular wrist
motion, until the contents are mixed.
(4) Place the vial in the preheated COD reactor. Reflux for 2 hours at 1500C.
(5) Allow the vials to cool then measure their absorbance in the HACHTIVI DR/1
Colorimeter. .
Standard Deviatio"n, 3mg/L

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 12

Ill. Physical Characteristics, cont.
9. Particulate Organic Carbon
Method 3. 1, A Manual of Chemical and Biological Methods for Seawater Analysis,
Parsons, Malta, and Lalli. 1984.

Reagents

(1) Sulfuric.Acid Dichromate 4.84g of K2Cr2O7 in 20ml of dl water. Add this
solution, a little at a time, to approximately 500ml of concentrated sulfuric acid. Cool
to room temperature and bring the total volume up to one liter with more concentrated
sulfuric acid in a volumetric flask. Warning... this reagent is particularly caustic.
(2) Phosphoric Acid : Analytical grade 70% phosphoric acid.
(3) Sodium Sulfate Solution : Dissolve 45g of anhydrous Na2SO4 in 1000ml of di water.
(4) Stock Glucose Solution Dissolve 7.50g of pure glucose, and a few crystals of HgC12,
in distilled water and bring up to a final volume of 100ml. The solution is stable for
many months in a refrigerator, bit should be discarded if any turbidity results.
(5) Standard Glucose Solution : Dilute 1 0.0ml of Stock Glucose Solution to 1 L in dl
water, 1.00ml=100gg of carbon.

Procedures

(1) Place a WhatmanO 4.25cm dia. 934-AH glass microfibre filter, in the Millipore@
filter apparatus. Attach a controlled vacuum source not exceeding 1/3 atmosphere.
After filtration of a suitable volume of sample, usually 0.51- to 2.OL, apply full suction
to the filter. Release'the suction after 1 minute, add 2ml of the sodium sulfate reagent,
and reapply the suction immediately ; repeat this process once more with 2ml of sodium
sulfate and remove the filter under suction.
(2) Place the filter into the bottom of a 50ml.beaker. Add 1.0ml of phosphoric acid and
1.0ml of distilled water. Mix and place into a block heater at 100-1100C for 30
minutes. Cover with a watch glass during this period.
(3) Add 10ml sulfuric acid-dichromate oxidant and 4ml of di water.
(4) Mix by swirling and place replace watch glass cover. Heat for 60 minutes at 100-
i i 00C.
(5) Allow the mixture to cool. Transfer the solution and the filter pad to a 50ml
graduated cylinder. Rinse the sides of the beaker beaker with di water. Add this wash to
the cylinder. Stopper and mix by inverting. ; allow solution to cool, and the filter should
settle on the bottom.
(6) Measure the extinction of the blank against the sample at 440nm. As the blank will
have a higher absorbance than the sample, the normal placement of samples in the
spectrophotometer will need to be reversed. Zero the sample against air.

Calculations

To determine the particulate organic carbons by this "wet ashing" technique
there must be a comparison of the decrease in the extinction of the sample solutions with
known standards. Prepare these standards, bringing them up to a volume of 50ml with

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 13

dl water, use them to calibrate every run of samples, and plot a concentrations versus
absorbance curve. Calculate sample concentrations from the slope of the standard line.

Standard Number -ml standard glucose mg C
1 0 0
2 1.0 0.30
3 2.0 0.60
4 3.0 0.90
5 4.0 1.20
6 5.0 1.5
7 10.0 3.00

10. Particulate Organic Matter
This is the same as the Total Suspended Volatile Solids. Method Number 209 D,
Standard Methods for the Examination of Water and Wastewater, Sixteenth Edition,
1985.

11. Total Alkalinity titration to an endpoint of pH4.5
Method Number 310.1, Methods for Chemical Analysis of Water and Wastes, EPA, 1983.

Procedure

Sample should be stored at 40C and run as soon as possible. Do not open the sample
bottle before analysis. Use a large volume of titrant for greatest accuracy, but keep
volume low enough to assure a sharp endpoint. Place sample in flask by pipetting with
the pipet tip near the bottom of the flask. Add standard acid while stirring with a Teflon
coated magnetic stirrer. Allow the pH meter to obtain equilibrium. Keep the air space
above sample to a minimum, the electrode and buret in contact with the sample may be
covered with parafilm or inserted through a rubber stopper. Titrate to a pH of 4.5.
Record the volume of titrant.

Reagents

(1) Sodium Carbonate Solution : 0.05N, 2.5 + 0.2g Na2CO3 dissolved in dl water in a 1 L
volumetric flask. The sodium carbonate must be dried at 250'C for 4 hours and cooled in
a dessicator prior to weighing.
(2) Standard Acid : OAN, HCI, or H2SO4. Dilute 3.Oml conc. H2SO4 or 8.3ml conc. HCI
to 11- with dl water. Standardize with 40ml of 0.05N Na2CO3 solution with about 60ml
of dl water by titrating potentiometrically to pH 5-. Lift the electrode and rinse it off
into the beaker. Boil the solution gently for 3-5 minutes under a watch glass cover. Cool
to room temperature. Rinse the cover'off into the solution. Continue the titration to the
endpoint.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 14

Calculations

Normality, N A x B
53.00 x C
A grams Na2CO3 weighed into 1L
B.= ml Na2CO3 solution
C ml acid used to reach endpoint

Alkalinity, mg/L CaC03 D x N x 50.000
Z
D = ml of standard acid
N = normality
Z = ml of sample
Standard Deviation 3.Omg/L Calcium Carbonate.

12. Chlorophyll
Method 4.1, A Manual of Chemical and Biological Methods for Seawater Analysis. T.
Parsons, Y. Maita, C. Lalli, Pergamon Press, 1984.

A known volume of seawater is filtered onto a synthetic filter or onto a glass
fiber filter; pigments are extracted from the filter in 90% acetone and their
concentration is estimated spectrophotometrically.
Between 0.5 and 1 liter of seawater are filtered through a membrane or glass
fiber filter (pore size .45 u). As the seawater is being filtered, a few drops of a
suspension of magnesium carbonate in seawater are added to prevent acidity on the filter.
The filter is drawn dry, removed, and can be folded and stored in a desiccator at -200C
for a least 30 days if.analysis can not proceed immediately. Filters should be folded in
half, backed with a piece of ordinary paper and fastened with a paper clip for storage.

Reagents

(1) 90% acetone: With a graduated cylinder measure 100ml of di water into a 1000ml
volumetric flask. Bring the volume of liquid in the flask to 1000ml with analytical
grade acetone.The reagent needs to be stored in a tightly stoppered bottle in the dark.
(2) Magnesium Carbonate: Add 1 g of powdered MgC03 to 1 00ml of dl water, and shake
vigorously.

Procedure

(1) Invert a polyethylene bottle containing the seawater sample into the Millipore
filtering equipment containing a membrane or fiber glass filter. Allow the sample to
filter under 1/2 atmosphere pressure vacuum.
(2) Add several (3 to 5) drops Of MgC03 solution to the seawater as it is being filtered.
(3) Drain the filter thoroughly with the suction and store or extract as necessary.

-1

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 15

(4) Place the filter in a 15-ml centrifuge tube; add 15ml of 90% acetone to volume and
shake thoroughly. Allow to stand overnight in a dark place (preferable refrigerated).
(5) Centrifuge the contents of each tube at room temperature for 5 to 10 min--the
exact time depending on the model of centrifuge and the degree of clarity obtained
(optical density at 750 nrn should be less than 0.05 in a 10-cm cuvette.
(6) Decant the supernate into a 10-cm path length spectrophotometer cuvette and
measure the extinction at the following wavelengths without delay (sample should be at
room temperature to avoid misting on the optical cell).

Wavelengths: 750, 664, 647, and 630.

(7) Correct each extinction for a small turbidity blank by subtracting the 750 nm
from the 664, 647, and 630 nrn absorptions. (The 510 nm absorbance is corrected by
subtracting 2X and 750 nm absorbance.)

Calculations

Calculate the amount of pigment in the original seawater sample using the equations
given below:

Ca = Chlorophyll a = 11.85 E664 - 1.54 E647 - 0.08 E630
Cb = Chlorophyll b = 21.0.3 E647 - 5.43 E664 - 2.66 E630
Cc Chlorophyll c = 24.52 E630 - 1.67 E664 - 7.60 E647

where E stands for. the absorbance at different wavelengths obtained above (corrected by
the 750 nm reading) and Ca, Cb and Cc are the. amounts of chlorophyll (in gg/ml if a 1-
cm light path cuvette is used); then:

ma chlorophyll Q x y
M3 V X 10

where v is the volume of acetone in ml (15 ml), V is the volume of seawater in liters
and Ca, Cb, and Cc are the three chlorophylls which are substituted for C in the above
equation, respectively (Note gg/1 mg/m3).

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 16

IV. Nutrients
(analyzed in the our Chemistry Laboratory)

1. Nitrogen, semi-micro Kjeldahl
Method Number 420 B, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.

Reagents

(1) Absorbant solution, plain boric acid: dissolve 20g H31303 in dl water and dilute to

(2) Borate buffer solution: 88ml OAN NaOH ( or 4.Og NaOH in 88ml dl water to about
500ml of 0.025M sodium tetraborate (9.5g N213407 -I OH20/L) and dilute to 1L.
(3) Digestion reagent: 134g K2SO4 in 650ml dl water and 200ml conc. H2SO4. Add,
while stirring, 25ml mercuric sulfate solution. Dilute the combined solution to 1 L with
water. Keep at a temperature close to 20 degrees C. to prevent crystallization.
(4) Sodium hydroxide - sodium thiosulfate reagent: 5OOg NaOH and 25g Na2S203
-51-120 in water and dilute to 1 L.
(5) All reagents for the determination of Ammonia by Nesslerization.

Procedure

Determine desired sample size based on the following table:
Organic Nitrogen Sample Size
in sample mg/L mL

4-40 50
8-80 25
20-200 10
40-400 5

(1) Transfer 50ml of sample, or an appropriate volume diluted to 50ml with
ammonia-free water to a 125ml erlenmeyer flask
(2) Add 3ml borate buffer solution and adjust pH to' 9.5 with 6N NaOH using a pH meter.
Quantitively transfer sample to a 100ml Kjeldahl flask and boil off 30ml. This removes
the ammonia. Skip this step if removal of ammonia is not desired.
(3) Add 10ml of digestion reagent to the sample in the Kjeldahl flask. Add 5 or 6 glass
beads (3-4mm diameter). Set heat on the Kjeldahl digestion rack on medium, boil
briskly under hood until solution clears (a pale straw color is acceptable) and copious
fumes are observed, usually about 30 minutes. Now turn heat up to the maximum
setting and digest for an additional 30 minutes. Cool.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 17

(4) Quantitatively transfer digested sample by diluting and rinsing into a rapid
distillation unit so that the total volume does not exceed 30ml. Add 10ml of hydroxide'
thiosulfate reagent.
(5) Adjust rate of steam in rapid, distillation unit so that there is no escape of steam
from the tip of the condenser or bubbling of contents of the receiving flask. Distill and
collect 30-40ml distillate below surface of 10ml boric acid solution contained in a
125ml distillate erlenmeyer flask. Extend tip of condenser well below level of the boric
acid solution and do not let temperature in condenser rise above 290C. Lower collected
distillate free of contact with delivery tube and continue distillation during the last 1 or
2 minutes to cleanse condenser.
(6) Carry a blank through the procedure.
(7) Determine ammonia by nesslerization.

Standards for Kleldahl Nitrogen (do not go through step 2)
Standard No. ml Standard Ammonia Conc. (mg/1)
1 0 0
2 0.5 0.122
3 1.0 0.244
4 2.0 0.488
5 4.0 .1.220
6 5.0 2.440'

2. Nitrogen, Nitrate, Cadmium Reduction
Method Number 418 C, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.

Reaaents

(1) Nitrate-free water: blank not to exceed 0.01 absorbance units.
(2) Copper-cadmium granules: Wash 25g of 40-60 mesh Cd granules with 6N HCI and
rinse with water. Swirl Cd with 100ml of 2% CuS04 solution for 5 min. or until blue
color partially fades. Decant and repeat with fresh CuS04 until a brown colloidal
precipitate develops. Wash Cu-Cd granules 10 times with water to remove all-----
precipitated Cu.
(3) Sulfanilmide reagent: dissolve 5g of sulfanilimide in a mixture of 50 ml conc. HCl
and 300ml dl water. Dilute to 500ml with dl water.
(4) N-(l-naphthyl)-ethylenediamine dihydrochloride solution: 500mg NED
dihydrochloride in 500ml water. Store in a dark bottle, replace
monthly and make a new calibration with each batch.
(5) Ammonium chloride-disodium ethylene diamine tetra-acetate solution: 26g NH4CI
and 3.4g EDTA in 2L of dl water. Add 1.3L of dl water and approximately 4.5ml NH40H
to bring to pH 8.5.
(6) Hydrochloric aci& 6N HCl
(7) Copper sulfate, 2%: 20g CuS04 5 H20 in 500ml H20, then dilute to 1L.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 18

(8) Stock nitrate solution: Dry KN03 in an oven at 105-C for 24 hours. Dissolve
0.7218g and dilute to 1 liter. Preserve with 2ml CHC13/L, 1ml = 100.0 gg N03--N.
This solution is stable for at least six months.
(9) Standard nitrate solution:: Dilute 50.Oml stock nitrate solution to 500 ml with
water. 1.00ml = 10.0 gg N03--N.
(10) Stock Nitrite Solution: 0.6072g KN02 (dried in a dessicator for 24 hours) is
dissolved in nitrite-free water and diluted to 1L. 1.00ml = 100 Rg N02--N. Preserve
with 2ml CHC13 and refrigerate. It is stable for 3 months.
(11) Standard Nitrite Solution: 50.0ml stock diluted to 500ml with nitrite-free
water. 1.00ml = 10.0 gg N02--N.

P roced u re

(1) Preparation of reduction column:
Insert glass wool plug and fill
column with water. Add CuCd
granules to a height of at least
18.5cm. Keep water over column
to prevent entrapment of air.
Wash column with 200ml of, dilute
NH4CI-EDTA. Activate column by
passing through it, at 7 to 10mis
per minute, 100ml of a solution
of 25ml of a 1.Omg N03-N/L
standard and 75ml NH4CI-EDTA
solution.
(2) Turbidity removal: if necessary
filter through either a 0.45gm
membrane or glass fiber filter.
(3) pH adjustment: adjust pH to 7-9 with dilute HCI or NaOH.
(4) Sample reduction: to 25.Oml of sample or a portion diluted to 25.0 ml, add 75ml
NH4CI-EDTA solution and mix . Pour into column and collect at a rate. of 7-1 Oml/min.
Discard first 25ml. Collect the rest in the original sample flask. There is no need to
wash column between samples, but if column is not to be used for several hours or
longer, pour in 50ml of dilute NH4CI-EDTA solution, letting it pass through system.
Store column in the solution; never let it dry out.
(5) Color development: As soon as possible a,nd not more than 15 minutes after
reduction, add 2.Oml sulfanilimide reagent to 50ml sample. Let react for 2-8 min. Add
2ml NED-dihydrochloride solution and mix immediately. Measure absorbance at 543nm
(after 10 min. but before 2 hours) against a distilled water-reagent blank.
(6) Standards: Dilute the following volumes of standard nitrate solution to 25ml with
dl water, and add 75ml of dilute Ammonium-Chloride-EDTA solution. Compare at least
one N02- standard to,the N03- to verify column efficiency.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 19

Standards for Nitrate
Standard No. ml Standard Nitrate Conc. (m /I
1 0 0
2 0.2 0.08
3 0.5 0.20
4 1.0 0.40
5 2.0 0.80
6 5.0 2.00
7 10.0 4.00

Calculations

Compute sample concentration directly from the standard curve, report as mg
oxidized N (N03- plus N02-) per liter. Subtract nitrite results to give figures for
nitrate.
Application Range = 0.01 to 1.0 mg/L'

3. Nitrogen, Nitrite Analysis
Method Number 419, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.

Reagents

(1) Nitrite-free water: Add a crystal of KMnO4 to 1 L distilled water. Discard initial
50mls. Collect the fraction that is free of permanganate, which gives a red color with
DPD reagent.
(2) Sulfanilimide reagent: Dissolve 5g of sulfanilimide in a mixture of 50ml conc. HCl
and 300ml distilled water. Dilute to 500ml with water. Stable.
(3) N- (I -nap hthyl) -ethy le nediarn in e-dihydroch to ride solution: Dissolve 500mg
NED dihydrochloride in 500ml of water. Store in the dark. Replace monthly or as soon
as a brownish color develops in the solution.
(4) Hydrochloric acid: HCI, 1 + 3.
(5) Sodium oxalate: 3.350g in 1000ml water.
(6) Ferrous ammonium sulfate: 19.607g plus 20ml conc. H2SO4 dilute to 1L with dl
water. This has to be standardized daily with a potassium chromate solution and ferroin
indicator.
(7) Stock nitrite solution: 1.232g of NaN02 in water and dilute to 1000ml. 1.00ml
250 micrograms.
(8) Standardize stock solution: Pipette in order: 50.00ml std. 0.05N KMn04; 5ml
conc. H2SO4, and 50.Oml stock N02. Shake gently and warm to 70-80'C. Discharge
permanganate color with standard FAS solution in 10ml portions. Titrate excess with
0.05M KMN04 to a faint pink endpoint. Carry a water blank through the entire
procedure.
9/1)

CHOCTAWHATCHEE - S. 0. P.
Date 12113/89
Page Number 20

A content of stock solution = r( B x C D x E
F
A = mg total N02- in the stock solution
B = total ml standard KMn04 used
C = normality of standard KMnO4
D = total ml standard reductant used, FAS
E = normality of standard reductant used, FAS
F = ml stack NaN02 solution taken for titration

jEach 1.00ml of 00.05N KMn04 corresponds to 350gg N02-

(9) Intermediate nitrite solution: G = 12.5/A. Dilute G (approximately 50ml) to
250ml with water. 1ml = 50.0 gg N. -Prepare daily.
(10) Standard nitrite solution: Dilute 10.00ml intermediate N02- solution to 1000ml
with water. 1.00ml = 0.500 micrograms N.
(11) 0.05N KMn04: 0.8g KMn04 per liter dl water. Keep in brown glass and age for
one week. Decant supernate without disturbing sediment and standardize supernate with
0.05N ferrous ammonium sulfate solution.
(12) Ferroin indicator: dissolve 1.485g 1,10-phenanthroline monohydrate and
695mg FeS04 -7H20) in dl water and dilute@to 100ml.
(13) FAS titrate: 0.25M. Dissolve 98g Fe(NH4)2(SO4)2-6H20 in dl water. Add
20ml conc H2SO4, cool and dilute to 1 000ml.
(14) Standard potassium dichromat,e: 0.0417M. Dissolve 12.259g K2Cr2O7, primary
standard grade, previously dried at 103'C for 2 hours, in dl water and dilute to 1L.
Standardize K2Cr2O7 daily by diluting 10ml of standard K2Cr2O7 to 100ml. Add 30ml
conc. H2SO4 and cool. Titrate with FAS titrate using 0.10 to 0.15ml (2 to 3 drops) of
ferroin indicator.
Procedure
(1) Filter sample through a 0.45 g membrane filter.
(2) To 50ml sample neutralized to pH 7.0, add Iml sulfanilimide reagent and let it
react for 2-8 minutes.
(3) Add 1.0ml NED dihydrochloride solution and mix immediately. Let stand at least 2
minutes but no more than 2 hours.
(4) Measure absorbance at 543nm.
Standards for Nitrite
Standard No. ml Standard Nitrite Conc. (m /I
1 - 0 0
2 0.1
3 0.2 0.002
4 0.4 0.004
5 0.7 0.007
6 1.0 0.010
7 2.0 0.020

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 21

Calculations

mg N02-/L 9 N02- (in 52ml final volume)
ml sample

4. Ammonia, Ion sensitive Electrode
Method Number 417 E, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985, and, Ammonia Combination Electrode, Corning Glass Works
Operating Instructions/Technical Specifications

Reagents

(1) Ammonia-free water
(2) Sodium Hydroxide, 6N. 240g of NaOH pellets in 10OOmL of dl water. This is
exothermic , allow solution to cool to adjust final volume to 10OOmL.
(3) Stock ammonium chloride solution, see Ammonia Nesslerization, reagent 4.
(4) Standard ammonium chloride solution, see Ammonia Nesslerization, reagent 5.

Procedure

(1) Prepare standards for Ammonia in a 125 erlenmeyer flask.
Standards for -Ammonia
Std. Number ml Std. Ammonia Concentration, ppm
0 0
2. 0.2 0.049
3 0.5 0.122
4 1.0 0.244
5 2.5 0.610
6 4.0 0.976
7 10.0 2.400

(2) Prepare Samples by pouring out 50mL into a clean 50mL erlenmeyer flask. be
sure to observe proper preservation proceedure for the samples prior to analysis.
(3) Equilibrate both samples and standards in the acid range with dilute HCI to pH 2.
This is unneccessary for samples that have been preserved properly. Also make sure
that both the samples and the standards are at the same temperature.
(4) Connect the Ammonia ISE to its imput connectors. With -the pH Meter in standby
turn the mode switch to -mv and begin calibration. Start on the blank, and add 1 mL of
6N NaOH to bring the pH above 11. With stirring on a magnetic stirrer with a teflon
stir bar zero the Meter to the blank. Then proceed to the standards of greater strength.
Measure ammonia content as one adds the NaOH, any delay may cause the loss of Ammonia
from the solution as soon as it is made basic. Always immerse the probe at an angle so
that gas does not get.-trapped on the tip. 300 is usually sufficient. Do not stir the
solution so violently that air is mixed in the solution. Always allow 2-3 minutes for the
mv reading to stabilize.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 22

(4) Remove the electrode and rinse with a small amount of sample. Immerse the
electrode into the sample with gentle stirring. Add 1 mL of 6N NaOH. Take a mv reading
when the display is stable, usually 1-2 minutes.
(5) Construct a curve from the standards on four-cycle semilog paper with
concentration in ppm on the log axis and mv on the linear axis.
(6) When not in use rinse the electrode in di water and blot it dry. Immerse the
electrode in 0.05M Ammonium Chloride. The membrane can be maintaned in such a
manner for 3-4 month.

5. Ammonia, Phenate Method
Method Number 417 C, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.

Reagents

(1) Ammonia Free Water
(2) Hypochlorous acid reagent: To 40 mL of di water add 10 mL 5% NaOCI solution
obtained from commercial chlorox bleach. Adjust to pH 6.5-7.0 with HCI. Reagent is
only stable for one week.
(3) Manganous Sulfate Solution, 0.006N: Dissolve 50 mg MnS04-H20 in 100ml- dl
water.
(4) Phenate Reagent: Dissolve 2.5g NaOH and 1 Og phenol in 1 OOmL dl water. This
reagent is only stable for one week. Handle Phenol with care.
(5) Stock ammonium chloride solution, see Ammonia Nesslerization, reagent 4.
(6) Standard ammonium chloride solution, see Ammonia Nesslerization, reagent 5.

Procedure

(1) 10 mL sample in a 50 mL erlenmeyer.
(2) Add one drop of Manganous Sulfate Solution.
(3) Place on a magnetic stirrer.
(4) Add 0.5 mL of Hypochlorous Acid Solution.
(5) Immediatly add 0.6 mL of Phenate Reagent, one drop at a time.
(6) Carry a blank and standards through the entire procedure
Standards for Ammonia
Std. Number ml Std. Ammonia Concentration, ppm
1 0 0
2 0.2 0.049
3 0.5 0.122
4 1.0 0.244
5 2.5 0.610
6 4.0 0.976
7 10.0 2.400

(7) Measure absorbanc'e at 630 nm. Color development is stable after 10 minutes, and
to 24 hours.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 23

6. Ammonia, Nesslerization
Method Number 417 B, Standard Methods for the Examinatiorz of Water and Wastewater,
Sixteenth Edition, 1985.

Reagents

(1) Zinc sulfate solution: dissolve 1 OOg ZnS04-7H20 and dilute tol L with ammonia-
free water.
(2) EDTA stabilizer: dissolve 50g of disodium ethylenediamine tetracetate dihydrate in
60ml of ammonia-free water containing 10g of NaOH, heat if necessary. Cool and dilute
to 100 mi.
(3) Nessler reagent: Dissolve 160g Hgl2. and 70g KI in a small amount of ammonia-
free water. Add slowly, with stirring,. to a solution of 160g NaOH in 500ml water.
Dilute to I L. Keep out of sunlight. Reagent keeps up to a year and can be checked by
development of the characteristic color with 0.1 mg NH3-N/L within 10 min. without
the development of a precipitate within 2 hours.
(4) Stock ammonia solution: Dissolve 3.819g anhydrous NH3CI (dry at 100'C) in
ammonia-free water, and dilute to 1 L. 1.00ml = 1.00mg N = 1.22mg NH3.
(5) Standard ammonium solution: Dilute 1 0.00ml no. 4 to 1 L with pure water.
1.00ml = 10.00gg N = 12.2gg NH3.
(6) Borate buffer: Add 88ml OAN NaOH solution to 500ml of 0.025M sodium
tetraborate solution (9.5g N313407-101-120/1-) and dilute to 1 L.
(7) Sodium hydroxide, 6N: Dissolve 240g NaOH in water and dilute to 1 L.

Procedure

(1) If interferences are noted, remove residual chlorine from the freely collected
sample, do not store chlorinated samples without prior dechlorination. Add 1ml ZnS04
solution to 100ml sample and mix. Add 0.4 to 0.5ml 6N NaOH to obtain a pH of 10.5.
Mix and let sample stand for a few minutes. A heavy, flocculent precipitate should form,
leaving the supernate clear and colorless. Filter or centrifuge sample. Pretest any.
filter paper with some nessler reagent to make sure it contains no ammonia. Filter
sample and discardthe first 25ml of filtrate. Samples containing more than 10mg NH3-
N/L may lose ammonia during treatment. Dilute such a sample to the sensitive range for
renesslerization before treatment.
(2) Use 50ml sample or a portion diluted to 50ml. If the sample contains high
concentrations of ions like calcium and magnesium that cause turbidity, or precipitate
with the nessler reagent, add 1 drop of EDTA reagent. Mix. Add 2ml of nessler reagent.
(3) Mix samples by swirling at least six times. Keep temperature and reaction time
constant in blank, samples and standards. Let the reaction proceed at least 10 minutes
after addition of the nessler reagent. If color development is weak use a 30 minute
contact time.
(4) Measure the absorbance at 425nm.

23.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 24

Standards for-Ammonia
Std. Number ml Std. Ammonia Concentration,
1 0 0
2 0.2 0.049
3 0.5 0.122
4 1.0 0.244
5 2.5 0.610
6 4.0 0.976
7 10.0 2.400
Detection Limit 1 gg Ammonia
M

24,

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 25

7. Phosphates, filtration
Filter samples through a 0.45 g membrane filter. Glass fiber filters may be used to
prefilter sample. Wash membranes by soaking in dl water to remove any residual
phosphates. To wash, soak 50 filters in 2L dl water for 1 hour. Change water and soak
for additional 3 hours.

filtration step: separates total and dissolved phosphate analysis

8. 'Phosphates, condensed phosphates
Method Number 424 B, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.

Reagents

(1) Phenolphthalein: aqueous solution
(2) Strong acid: add 300ml of conc. H2SO4 to about 600ml dl water. When cool add
4.Oml conc. HN03, dilute to 1 L.
(3) Sodium hydroxide: NaOH 6N, see Ammonia, Ion Sensitive Electrode, reagent 2.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 26

Procedure

(1) 50 mi sample
(2) Add 2 drops phenolphthalein, and acidify dropwise with the strong acid solution if a
red color ensues. Add another mi of acid after discharge of color to each sample.
(3) Boil gently for 90 minutes, being careful to keep sample volume at around 25-
50ml, or autoclave for 30 minutes at 98-137kPa with foil caps on the flasks. Cool and
neutralize to a faint pink color with 6N NaOH. Restore to original 100ml volume with dl
water.
(4) Run the phosphate standards through step number 3 to assure a good calibration
curve.
(5) Colorimetric method: run ascorbic acid test to quantitate.

9. Phosphates, total phosphate
Method Number 420 C, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.

Reagents

(1) Sulfuric acid: conc.
(2) Nitric acid: conc.
(3) Phenolphthalein: aqueous solution
(4) Sodium -hydroxide: 1 N NaOH

P roced u re

(1) Add 50ml sample to a micro-kjeldahl flask. Add 1 mi conc. H2SO4 and 5ml conc
HN03.
(2) Digest to a volume of 1 mi. Continue digestion to a discharge of color which signifies
the removal of HN08, approximately 40 minutes.
(3) Cool. Add about 20ml dl water. .
(4) Add 1 drop of phenolphthalein and as much 1 N NaOH as necessary to produce a faint
pink tinge.
(5) Transfer to erlenmeyer flask, with filtration (only if necessary), and adjust
samplevolume to 100ml with dl water.
(6) Colorimetric Method, run ascorbic acid.

10. Ortho-phosphates, ascorbic acid method
Method Number 424 F, Standard Methods for the Examination of Water and Wastewater,
Sixteenth Edition, 1985.

Reagents

(1) Sulfuric acid: 70ml conc. H2SO4 in 500ml water (5N) or 280ml in 2L.
(2) Potassium antimonyl tartrate solution: 1.3715g in'400ml water, and dilute to
500ml. Store in glass stoppered bottle.

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Nu'mber 27

(3) Ammonium molybdate solution: 20g in 500ml water. Store in glass stoppered
bottle.
(4) Ascorbic acid (0.01 M): 1.76g in 100ml dl water; stable for 1 week at 40C, or
2.64g in 150ml dl water, or 5.26g in 300ml dl water.
(5) Combin@@@
[100ml total] (500ml total] (1000ml total]
50ml 5N H2SO4 250MI H2SO4 500ml H2SO4
5ml PAT 25ml PAT 50ml PAT
15ml AM 75ml AM 150ml AM 30ml
IAA 150ml AA 3 0 0 rn I
(6) Stock phosphate solution: 219.5mg anhydrous KH2PO4 in1OOOml waterl ml 50
N P04
(7) Standard phosphate solution: dilute 50ml stock phosphate solution to
1000ml with water. 1ml "- 2.5 microgram P04

Procedure

(1) pour 50ml sample into a 125ml erlenmeyer flask
(2) add 2 drop phenolphthalein indicator
(3) if red color develops add 5N H2S04 dropwise until discharge of color
(4) add 8ml of the combined reagent and mix thoroughly
(5) after 10 minutes, but not before 3.0 minutes, measure absorbance at 880nm. Use a
reagent blank as the reference.

Standards for Phosphate
Standard No. ml Standard Phosphate Conc. (mg1I)
1 0 0
2 0.2 0.010
.3 0.5 0.025
4 1.0 0.050
5 5.0 0.250
6 10.0 0.500
7 20.0 1.000
Detection Limit 10 gg Phosphate

CHOCTAWHATCHEE - S. 0. P.
Date 12/13/89
Page Number 28

V. Solutions
1. Lugal's Solution, for preserving plankton samples

20g KI 60g KI
I Og 1, crystalline 30gl, crystalline
200ml dI H20 600ml dI H20
20ml Acetic Acid, glacial 60ml Acetic Acid, glacial
Note: Mix the di water with the glacial acetic acid first, then add the other ingredients
with stirring.

Dose:

0.3ml of Lugal's will preserve 100ml of sample if it is stored in the dark. For
long term storage use 0.7ml of Lugal's for 100ml of sample.

2. Bouin's Solution, for preserving histological samples

10 parts formalin
90 parts picric acid
1 part 1 +1 acetic acid

Note: The solubility of picric acid it water is 1g/78ml or 12g/L. Prepare the solution
with care. Dry crystalline picric acid is explosive when subjected to any impact, such
as dropping it on the floor. Jhis solution will fix the tissues of ones hand upon contact.

3. Probe Juice, for Y.S.I. D.O. Probes
Use half saturated KCI in dl water. A saturated KCI solution is used with the
Calomile Electrodes. Dilute, the saturated solution with one part water to get a half
saturated solution.

4. Probe Cleaner, for the Y.S.I. S.C.T. Probes
Any commercial foaming tile cleaner can be used, but it is best to use a home
brew cleaner of : 10 parts dl water; 10 parts isopropanol; and 1 part concentrated HCL

5. Probe Cleaner, for the Y.S.I. D.O. Probes
To clean the gold electrode rub its' surface with an abrasive eraser like those
used on ball point ink pens. To clean the silver electrode empty out the probe juice and
fill the chamber with 14% NH40H. Soak for 10 minutes. Rinse the chamber with
several volumes of dl water. Fill chamber with probe juice, and replace membrane.

all'-pendix III

Photographic Atlas, of Dominant Phytoplankton Species
f ound in the
Choctawhatchee Bay System

A note on Photomicrographs and legends

The present atlas is the continuation of the
previously prepared "An Atlas of diatoms and other forms from
selected Drainage areas in Central and North Florida" (Prasad
& Livingston 1987), and includes only those forms that
occur in brackishwater and marine environments. This atlas
is a photographic survey at the light microscopic level of
over 255 algal taxa belonging to 90 genera. The groups
represented here include Bacillariophyceae (Diatoms),
Chrysophyceae(Golden-brown algae), Cyanophyceae (Blue-green.
algae), and Dinophyceae (Dinoflagellates). The freshwater
atlas mentioned above contains illustrations for over 460
taxa belonging to 72 genera. These two works, together,
provide a comprehensive account of the algal species
present in river-bay systems

The micrographs were taken with two NIKON research
microscopes, one (LABOPHOT) being equipped for bright and
phase contrast illumination, the other (MICROPHOT)
exclusively for Nomarski Differential Interference Contrast
(DIC). Most of the photographs were taken with oil-immersion
phase,contrst objectives (10OX with 1-.25 numerical aperture
and 0.16 mm working distance). The DIC was used in cases
where valves lying on top of one another had to be seperated
optically. For e.g. in seperating valves of Achnanthes,
Cocconeis, Mastogloia etc. All micrographs were taken on
Pan-X black and white film and the prints and enlargements
were made on Kodak Poly contrast III RC multigrade
photographic paper.

The arrangement of photomicrographs in this atlas is
quite simple. The plates are arranged in different phyla or
divisions of generally accepted systems of classification.
The genera and species in each family represented are not
arranged. in any particular order. Each taxon is illustrated.
by more than one figure reflecting therange of variability
from each locality and season. many species of diatoms that
are weakly silicified such as those of Chaetoceros and
Rhizosolenia were mounted in distilled water without
cleaning,th6m with acids. The legends for plates are kept
brief. Location and month of collection are included as notes
regarding the spacial and temporal occurrence of each taxon,
followed by the numerical magnification.