PRIMARY PRODUCTIVITY
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SUMMARY: The 14C-radiotracer method is used to measure
the assimilation of dissolved inorganic carbon (DIC) by
phytoplankton as an estimate of the rate of photosynthetic
production of organic matter in the euphotic zone.
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1. Principle
The 14C method, originally proposed by Steeman-Nielsen (1952),
is used to estimate the uptake of dissolved inorganic carbon (DIC)
by planktonic algae in the water column. The method is based on the
fact that the biological uptake of 14C-labeled DIC is proportional
to the biological uptake of 12C-DIC. If one knows the initial
concentration of DIC in a water sample, the amount of 14C-DIC added,
the 14C retained in particulate organic matter (14C-POC) at the end
of the incubation and the metabolic discrimination between the two
isotopes of carbon (i.e., 5% discrimination against the heavier 14C
isotope), then it is possible to estimate the total uptake of carbon
from the following relationship:
DIC * 14C-POC * 1.05
C uptake = --------------------
14C-DIC added
Due to the potentially toxic effects of trace metals on phytoplankton
metabolism in oligotrophic waters, the following procedure is used to
minimize the contact between water samples and possible sources of
contamination.
2. Cleaning
2.1. HCl (Baker Instra-Analyzed) solution (1M) is prepared with high
purity hydrochloric acid and freshly-prepared glass distilled
deionized water (DDW).
2.2. 500 ml polycarbonate bottles are rinsed twice with 1M HCl
(Baker Instra-Analyzed) and left overnight filled with the same
acid solution. The acid is removed by rinsing the bottles three
times with DDW before air drying.
2.3. Go-Flo bottles, fitted with teflon-coated springs, are rinsed
three times with 1M HCl and DDW before use.
2.4. Pipette tips used in the preparation of the isotope stock and
in the inoculation of samples are rinsed three times with
concentrated HCl (Baker Instra-Analyzed), three times with DDW
and once with the sodium carbonate solution (Chapter 14, section
3.2) and stored in a clean polyethylene glove until used.
3. Isotope Stock
3.1. The preparation of the isotope stock is performed wearing
polyethylene gloves. A 25 ml acid-washed teflon bottle and a
50 ml acid-washed polypropylene centifuge tube are rinsed three
times with DDW.
3.2. 0.032 g of anhydrous Na2CO3 (ALDRICH 20,442-0, 99.999% purity)
are dissolved in 50 ml DDW in the centrifuge tube to provide
a solution of 6 mmol Na2CO3 per liter.
3.3. 3.5 ml of NaH-14CO3 (53 mCi mmol-1; Research Products Inc.)
are mixed with 16.5 ml of the above prepared Na2CO3 solution
in the teflon bottle.
3.4. The new stock activity is checked by counting triplicate 10 µl
samples with 1 ml β-phenethylamine in 10 ml Aquasol-II.
3.5. Triplicate 10 µl stock samples are also acidified with 1 ml of
2 M HCl, mixed intermittently for 1-2 hours and counted in 10
ml Aquasol-II to confirm that there is no 14C-organic carbon
contamination. The acidification is done under the hood.
The acidified dpm should be <0.001% of the total dpm of the 14C
preparation.
4. Incubation Systems
Typically we measure primary production using in situ incubation
techniques.
4.1. A free-floating array equipped with VHF radio and strobe light
is used for the in situ incubations. Incubation bottles are
attached to a horizontal polycarbonate spreader bar which is
then attached to the 200 m, 1/2" polypropylene in situ line at
the depths corresponding to the sample collections.
4.2. Generally eight incubation depths are selected (5-175 m,
approximately).
5. Sampling
5.1. Approximately 3 hours before local sunrise, seawater samples
are collected with acid- washed, 12-liter Go-Flo bottles using
Kevlar line, metal-free sheave, teflon messengers and a
stainless steel bottom weight. A dedicated hydrowinch is used
for the primary productivity sampling procedures in a further
effort to reduce/eliminate all sources of trace metal contamination.
5.2. Under low light conditions, water samples are transferred to the
incubation bottles (500 ml polycarbonate bottles) and stored in
the dark. Polyethylene gloves are worn during sample collection
and inoculation procedures. No drawing tubes are used.
6. Isotope Addition and Sample Incubation
6.1. Three light bottles, three dark bottles and 1 time-zero control
(see Chapter 14, section 8) are collected at each depth for in
situ incubation. In situ dark bottles are deployed in specially-
designed, double-layered cloth bags with VelcroR closures.
6.2. After all water samples have been drawn from the appropriate Go-Flo
bottles, 250 µl of the 14C-sodium carbonate stock solution is added
to each sample using a specially-cleaned pipette tip. The samples
are deployed before dawn on a free-floating, drifter buoy array.
6.3. At local sunset, the free-floating array is recovered and all in
situ bottles are immediately placed in the dark and processed as
soon as possible. The time of recovery is recorded.
7. Filtration
7.1. Filtration of the samples is done under low light conditions and
begins as soon as the incubation bottles are recovered from the
in situ array.
7.2. 200 µl are removed and placed into a second LSC vial containing
0.5 ml of β-phenethylamine. This sample is used for the
determination of total radioactivity in each sample.
7.3. The remainder is filtered through a 25 mm diameter GF/F filters.
The filters are placed into prelabelled, clean glass liquid
scintillation counting vials (LSC vials) and stored at -20 °C.
8. 14C Sample Processing
8.1. One ml of 2 M HCl is added to each sample vial (under the hood).
Vials are covered with their respective caps and shaken in a
vortex mixer for at least 1 hour with venting at 20 minute
intervals. To vent, the vials are removed from the shaker,
and the cap opened (under the hood). After shaking is completed,
the vials are left open to vent under the hood for an additional
24 hours.
8.2. Ten ml of Aquasol-II are added per vial (including vials for total
14C radioactivity) and the samples are counted in a liquid
scintillation counter. Samples are counted again after 2 and
4 weeks, before discarding. Counts have shown a consistent
increase during the first two weeks and become stable between
the second and the fourth week. This is probably the result of
sample hydrolysis or diffusion of radioactivity from the GF/F
filter matrix, thereby reducing the extent of self-absorption.
Only the 4-week count is used for 14C calculations. Counts per
min (CPM) are converted to disintegration per min (DPM) using
the channels ratio program supplied by the the manufacturer
(Packard Instrument Co.).
9. Calculations
From the data derived above we can estimate several properties of
the phytoplankton populations at Station ALOHA. Total daylight organic
carbon production is calculated from the 12-hour uptake data (after
corrections for 12-hour dark activities). Net daily organic carbon
production is calculated from the 24-hour light/dark samples (corrected
for the time-zero blank activities). Phytoplankton population respiration
is taken as the difference between the 12-hour light and the 24-hour
light/dark incubations. Net primary production is used as the estimate
of phytoplankton carbon production for the purposes of comparison to
other ecosystem-level processes (e.g., standing stock assessments,
vertical C-flux, etc.).
10. Equipment/Supplies
Go-Flo bottles
kevlar hydroline
teflon messengers
stainless steel weight
temperature- and light-controlled deck incubation system
(NORDA/USM incubation system)
free-drifting productivity array (including polypro line,
spreader bars, surface floats, buoy, radio
transmitter and strobe le light)
500 ml wide-mouth polycarbonate bottles
vacuum filtration system
liquid scintillation counting (LSC) vials
pipettes
glassware
vortex mixer
liquid scintillation counter (Packard model 4640; United
Technologies Inc.)
11. Reagents
distilled deionized water (DDW)
HCl for trace metal analysis (Baker Instra-Analyzed)
Na2CO3 (99.999%)
NaH-14CO3 solution (cat #CMM-50, Research Products Inc.)
β-phenethylamine
Aquasol-II (Dupont)
2 M HCl
12. References
Steeman-Nielsen, E. 1952. The use of radioactive carbon (14C)
for measuring organic production in the sea. Journal du Conseil,
18, 117-140.
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