JoVE Biology

Establishment of Microbial Eukaryotic Enrichment Cultures from a Chemically Stratified Antarctic Lake and Assessment of Carbon Fixation Potential

1, 1, 1

1Department of Microbiology, Miami University

Article
    Downloads Comments Metrics Publish with JoVE

    You must be subscribed to JoVE to access this content.

    Enter your email to receive a free trial:

    Welcome!

    Enter your email below to get your free 10 minute trial to JoVE!


    By clicking "Submit", you agree to our policies.

    Admit it, you like to watch.

     

    Summary

    Microbial eukaryotes are both a source of photosynthetically-derived carbon and top predatory species in permanently ice-covered Antarctic lakes. This report describes an enrichment culture approach to isolate metabolically versatile microbial eukaryotes from the Antarctic lake, Lake Bonney, and assesses inorganic carbon fixation potential using a radioisotope assay for Ribulose-1,5-bisphophate carboxylase oxygenase (RubisCO) activity.

    Date Published: 4/20/2012, Issue 62; doi: 10.3791/3992

    Cite this Article

    Dolhi, J. M., Ketchum, N., Morgan-Kiss, R. M. Establishment of Microbial Eukaryotic Enrichment Cultures from a Chemically Stratified Antarctic Lake and Assessment of Carbon Fixation Potential. J. Vis. Exp. (62), e3992, doi:10.3791/3992 (2012).

    Abstract

    Lake Bonney is one of numerous permanently ice-covered lakes located in the McMurdo Dry Valleys, Antarctica. The perennial ice cover maintains a chemically stratified water column and unlike other inland bodies of water, largely prevents external input of carbon and nutrients from streams. Biota are exposed to numerous environmental stresses, including year-round severe nutrient deficiency, low temperatures, extreme shade, hypersalinity, and 24-hour darkness during the winter 1. These extreme environmental conditions limit the biota in Lake Bonney almost exclusively to microorganisms 2.

    Single-celled microbial eukaryotes (called "protists") are important players in global biogeochemical cycling 3 and play important ecological roles in the cycling of carbon in the dry valley lakes, occupying both primary and tertiary roles in the aquatic food web. In the dry valley aquatic food web, protists that fix inorganic carbon (autotrophy) are the major producers of organic carbon for organotrophic organisms 4, 2. Phagotrophic or heterotrophic protists capable of ingesting bacteria and smaller protists act as the top predators in the food web 5. Last, an unknown proportion of the protist population is capable of combined mixotrophic metabolism 6, 7. Mixotrophy in protists involves the ability to combine photosynthetic capability with phagotrophic ingestion of prey microorganisms. This form of mixotrophy differs from mixotrophic metabolism in bacterial species, which generally involves uptake dissolved carbon molecules. There are currently very few protist isolates from permanently ice-capped polar lakes, and studies of protist diversity and ecology in this extreme environment have been limited 8, 4, 9, 10, 5. A better understanding of protist metabolic versatility in the simple dry valley lake food web will aid in the development of models for the role of protists in the global carbon cycle.

    We employed an enrichment culture approach to isolate potentially phototrophic and mixotrophic protists from Lake Bonney. Sampling depths in the water column were chosen based on the location of primary production maxima and protist phylogenetic diversity 4, 11, as well as variability in major abiotic factors affecting protist trophic modes: shallow sampling depths are limited for major nutrients, while deeper sampling depths are limited by light availability. In addition, lake water samples were supplemented with multiple types of growth media to promote the growth of a variety of phototrophic organisms.

    RubisCO catalyzes the rate limiting step in the Calvin Benson Bassham (CBB) cycle, the major pathway by which autotrophic organisms fix inorganic carbon and provide organic carbon for higher trophic levels in aquatic and terrestrial food webs 12. In this study, we applied a radioisotope assay modified for filtered samples 13 to monitor maximum carboxylase activity as a proxy for carbon fixation potential and metabolic versatility in the Lake Bonney enrichment cultures.

    Protocol

    1. Sample Acquisition

    1. Choose and prepare the sampling site one day prior to sampling the water column. This will allow the stratified layers of the water column to reform after disturbance due to drilling and ice-hole melting. Identify location of drill site by GPS.
    2. To access the water column, begin by drilling a hole through the ice with a Jiffy ice auger attached to a 4-inch Jiffy flight extension and cutting bit. To prevent freezing of the drill in the hole, try to avoid drilling into the liquid water by halting drilling approximately 4-6 inches above the top of the water column.
    3. The drill hole will need to be widened from a diameter of 15 to 60 cm prior to sampling. This is accomplished by use of a hole melter (Hotsy Model) which circulates heated polyethylene glycol through a copper pipe. Hole melting typically takes up to 18 hours.
    4. Prior to sampling the water column, ensure that all required equipment and sample storage vessels are assembled at the sampling site. Sampling materials include: Niskin bottle (5-10 L capacity), Winch with depth-calibrated cable, Messenger, sufficient sample bottles for each sampling depth and coolers for sample transport.
    5. Begin sampling early in the day (~5 am), as lake water filtering should be completed on the day of sampling. Collect water samples (1-5 L) from desired depths (for this study: 6-m, 15-m and 18-m sampling depths, measured from the piezometric water level in the ice hole) using a Niskin sampler attached to a calibrated hand winch. To prevent disturbance of the water column collect shallow depths before deeper ones.
    6. Store lake samples in coolers and transport from the sample site to the field lab using a sled attached to an ATV (all terrain vehicle). Samples should be processed or stabilized (for eg: flash freeze in liquid nitrogen) at the field laboratory immediately following sampling.

    2. Development of Enrichment Cultures

    1. For cultivation of enrichment cultures,Concentrate 0.5-1 L of lake water onto 47 mm 0.45 μm pore size polyethersulfone filters using gentle filtration (< 0.3 atm). If the diversity of the natural community is desired, filter a second sample onto 47 mm 0.45 μm pore size polyethersulfone filters and follow protocols according to Bielewicz et al. 4 for eukaryote phylogenetic diversity.
    2. Transfer filter to 50 mL sterile falcon tube containing ~20 mL of filtered lake water collected from the same sampling depth as the filter. Gently wash cells from the filter using a sterile pipette.
    3. Transfer cell suspension to a 25 cm2 sterile cell culture flask. Add filtered lake water collected from each sample depth to increase the culture volume to 45 mL. Set up multiple replicates for each sampling depth if enrichments on different culture media are desired.
    4. Supplement culture flasks with 50X sterile solutions to a final concentration of 1X of the following culture media: Bold's Basal Medium, BG11 and F/2. If cultivation of mixotrophic organisms is required, set-up two F/2-supplemented vessels and add 2-3 grains of sterile rice to one of the flasks.
    5. Incubate culture flasks at low temperature (4 °C) and low irradiance (20 μmol photons m-2 s-1) in a temperature-controlled growth incubator for at least 4 weeks in Antarctica prior to shipment to your U.S. laboratory. If isolates are desired, plate 250 μL of enrichment culture on agar plates containing appropriate growth media after 2 weeks incubation.
    6. For shipment to the U.S., transfer enrichment cultures to sterile 50-mL falcon tubes. Request shipment requirement of "do not freeze" and "keep cool" on shipping request. While the shipping process from Antarctica is relatively fast (2 weeks by commercial air) and highly reliable, there is a possibility of loss of fastidious organisms during the transport process. Thus, investigators may want to preserve a subsample prior to shipping so that loss of certain species during the shipping process can be assessed.
    7. Upon arrival in the U.S., transfer 5 mL of enrichment culture into 45 mL of appropriate growth media in a 125-mL sterile Erlenmeyer flask capped with a sterile sponge. Enrichment cultures should be maintained as standing cultures in a temperature controlled environmental growth chamber (Diurnal Growth Chamber, VWR) at 4 °C/20 μmol photons m-2 s-1. Cultures should be transferred to fresh media every 30 days.

    3. Cell Lysate Extraction from Filtered Enrichments

    1. Filter 5 mL of enrichment culture onto a 25 mm Whatman GF/F filter using gentle vacuum (<10 psi). The filter may be stored for several weeks at -80 °C prior to assaying RubisCO activity.
    2. Cut the filter into 4-5 sections with sterile steel scissors and transfer the pieces with sterile forceps to a 2 mL screw cap tube filled one fifth of the way full with 0.1 mm diameter zirconia/silica beads.
    3. Add 1.25 mL of filter extraction buffer (50 mM bicine, 10 mM MgCl2, 1 mM EDTA, 5 mg/mL BSA, and 0.1% triton X-100; add fresh: 10 mM NaHCO3, 10 mM DTT, 3.3 mM aminocaproic acid, 0.7 mM benzamidine, pH 7.8) 13 and disrupt cells using a Minibead beater three times for 30s on speed setting 48. To prevent heating of the sample, alternate beadbeating with 1 min ice incubation.
    4. Centrifuge filter slurry for 2 min at 3000 x g at 4 °C to form a loose pellet of GF/F filter fibers and cell wall debris.
    5. Remove a 200 μL aliquot and immerse in 800 μL of ice-cold 90% acetone. Measure extractable chlorophyll (chl) a in a spectrophotometer at wavelength values of 664 nm and 647 nm 14. Transfer the supernatant to a 1.5 mL microcentrifuge tube.
    6. Centrifuge remaining supernatant at 4 °C for 2 min at 15,000 x g and transfer the supernatant (avoid the pellet of insoluble cellular membranes and remaining GF/F filter fibers) to a clean 1.5 mL microcentrifuge tube. This soluble cell lysate may now be used in the RubisCO carboxylase activity assay.
    7. Lysate may be stored at -80 °C after addition of 12.5% glycerol and flash freezing in liquid nitrogen A loss of activity may occur after multiple freeze/thaw cycles depending on the sensitivity of the enzymes in the lysate. Therefore, activity of fresh versus frozen lysate should be tested before large scale cell lysate extractions.

    4. RubisCO Carboxylase Activity Filter Assay

    1. Transfer 125 μL of soluble lysate to a 15 mL screw cap microcentrifuge tube (cap not needed) that has been chilled on ice. For negative control samples, add 125 μL soluble lysate to 15 mL screw cap microcentrifuge tube, but do not add substrate (in step 4.7). Run duplicate reactions for all samples and negative controls.
    2. Prepare 10 mL of assay buffer fresh (50 mM Bicine-NaOH, pH 8.0, 50 mM NaHCO3, 25 mM MgCl2) and chill on ice. Aliquot enough of the assay buffer for all of the samples and negative controls (100 μL per sample/control plus 100 μL extra) to a 5 mL tube. Perform all subsequent steps under a fume hood.
    3. Add 40 μL NaH14CO3 (500 μCi/mL) per mL of assay buffer to the aliquoted buffer and keep the buffer on ice.
    4. Remove 10 μL of the assay buffer containing 14C and dilute it in 1 mL of assay buffer. After inverting to mix, add 100 μL of the 1:100 diluted mixture to 3 mL of Bio-Safe II scintillation counting cocktail in a scintillation vial. Invert to mix. Scintillation counts (Beckman LS6500) should be over 18,000 cpm before continuing with the assay.
    5. When enough NaH14CO3 has been added to the assay buffer, move the reaction tubes to a dry bath preset to 25 °C and incubate for 3-5 mins.
    6. Add 100 μL assay buffer to the lysates and incubate for 5 mins at 25 °C.
    7. Add 20 μL of 15 mM Ribulose bisphosphate, to samples and allow the reaction to proceed for 5-10 mins at 25 °C.
    8. Add 100 μL propionic acid (100%) (Fisher) to stop the reaction. Centrifuge for 1 hour at 2,000 x g to exhaust unincorporated 14C.
    9. Transfer the total volume of the samples to scintillation vials containing 3 mL Bio-Safe II scintillation counting cocktail. Determine cpm of acid stable end products by scintillation counting (B. Witte, R. Tabita personal communication).
    10. Calculate RubisCO activity rates on a chl a basis 14.

    5. Representative Results

    We utilized enrichment culturing to isolate cold-adapted phototrophic and mixotrophic protists residing in the Antarctic Lake Bonney. To capture a greater diversity of organisms, we tested three growth media types: Bold's Basal Medium (BBM) 15, F/2-Si Marine Medium 16, 17 and BG11 Medium 18. Visual inspection of the enrichment cultures by light microscopy revealed that the cultures were dominated by phototrophic protists (indicated by the presence of chlorophyll pigment in most cells) and harbored a variety of cell morphologies depending on the sampling depth from which the inoculum was taken and the type of media used in the culture (Fig. 1).

    We measured maximum rates of carboxylase activity catalyzed by the enzyme RubisCO as a proxy for carbon fixation potential. Chl a abundance was also monitored as an estimate of phototrophic protist biomass (Fig. 2). Despite cultivation of all cultures under the same temperature/light regime (ie. 4 °C/20 μmol m-2 s-1), carbon fixation potential and phototrophic biomass varied dramatically between the enrichment cultures. Maximum RubisCO activity was observed in enrichment cultures growing in either BBM (Enrichments 4 and 6) or BG11 (Enrichments 13 and 14) growth media, while cultures enriched on F/2 growth medium (Enrichments 19, 21, 23) exhibited a 4- to 34-fold lower maximum carboxylase activities. These differences were not due to lower biomass levels in the F/2 cultures, as carboxylase activity was expressed on a Chl a basis. Moreover, RubisCO activity did not correlate with chl a concentration (r = -0.023, p>0.1; Fig. 2, inset). The BBM cultures inoculated with lake water from 6 m and 15 m (Enrichments 4 and 5) had the highest chl a levels, while all other cultures exhibited relatively low chl a, regardless of RubisCO enzyme activity (Fig. 2).

    Figure 1
    Figure 1. Representative microbial eukaryote enrichment cultures which have selected for the growth of different organisms. Identity of the culture is given in the lower left of the panels. All images represent light micrographs generated using oil immersion at 1000X magnification.

    Figure 2
    Figure 2. Potential carbon fixation capacity and extractable chlorophyll a levels in Antarctic microbial eukaryote enrichment cultures isolated from Lake Bonney and grown on various culture media. See Table 1 for culture details. Inset: Pearson correlation between chlorophyll a abundance and carbon fixation potential in Antarctic microbial eukaryote enrichment cultures.

    Subscription Required. Please recommend JoVE to your librarian.

    Discussion

    Recent molecular studies have reported high diversity of single-celled eukaryotes across a range of environments 3, 19, 20; however, due to a lack of isolates across the full range of protist habitats the functional roles of these individual species in food webs are largely unknown. In this study, we have described methodologies to enrich for microbial eukaryote species exhibiting metabolic versatility from a relatively undersampled environment, a permanently ice-covered Antarctic lake. Cultures enriched from different sampling depths in Lake Bonney exhibited differential carbon fixation rates that were growth medium-dependent. For example, low carbon fixation potential in cultures enriched in F/2 versus BBM or BG 11 growth media likely reflects differences in protist diversity and metabolic capability. BBM growth medium selects for green algal species (or chlorophytes) and our cultures appear to be a monoculture of a green algal species (Fig. 1A, B). These organisms are known to largely depend on photoautotrophy. One isolate from Lake Bonney exhibits pure photoautotrophic metabolism, having a strict requirement for light as its sole energy source 1. In contrast, F/2 growth medium is designed to enrich for a broad range of marine protists, including potentially mixotrophic organisms 12. While we did not fully explore the diversity of the F/2 cultures, microscopic views of these enrichments clearly show a consortium of protists of various cell morphologies (Fig. 1C, D). Thus, reduced RubisCO activity in the F/2 cultures could be due to utilization of alternative carbon/energy acquisition modes. In support of this prediction, pure cultures of photoautotrophic Antarctic isolates exhibit significantly higher maximum RubisCO carboxylase rates compared with Antarctic isolates that exhibit mixotrophy (Dolhi & Morgan-Kiss, unpublished results). Further studies of heterotrophic enzyme activity in these samples would help to fully characterize the metabolic versatility of the protist enrichment cultures and are currently underway in our laboratory. In addition, the physiological data described in this paper will be complemented with phylogenetic and metagenomic sequencing information as part of a large sequencing effort to characterize microbial communities across the globe called the Earth Microbiome Project (http://www.earthmicrobiome.org/).

    The modified filter assay described in this report could also be applied to cell lysate extracted from filtered lake water samples. However, for new applications of this assay, optimal lysate volume should be determined by assaying three different volumes and using that which yields cpm at least 3 to 4 times above the negative controls. Analyses of carbon fixation potential in conjunction with enzymatic analyses of heterotrophic activity in natural protist communities would provide a more detailed view of the role of protist trophic ability and carbon cycling in aquatic environments. We are currently applying this approach to understand the role of abiotic environmental factors in protist metabolic versatility in Lake Bonney and other Antarctic lakes. The RubisCO carboxylase filter assay method will be a valuable tool to study potential carbon fixation and metabolic versatility in small scale enrichment cultures as well as whole lake systems.

    Prior to the development of cultivation independent molecular tools, protists were traditionally identified by cultivation and taxonomically classified based on their cell morphology. Thus, there is a long history of enrichment and isolation of protists residing in a wide variety of habitats. Early investigations in particular are historically valuable for detailed taxonomic identification (reviewed in: 21, 22). While isolation of protists using enrichment-based approaches is relatively rare in Antarctic freshwater environments, several marine protist isolates from enrichment of Antarctic seawater are available 23-26. In addition, several culture collections are dedicated to protist and microalgal isolates (for eg: the Provasoli-Guillard culture collection, https://ncma.bigelow.org/). Dependable and cheap sequencing technologies have produced a massive genetic database of uncultivated protistan sequences. While these databases have been very informative regarding the diversity and distribution of this important group of microorganisms, there is a widening gap in linking sequence data with our understanding of the protist ecology and physiology. Thus, traditional cultivation techniques, particularly in undersampled environments such as polar aquatic habitats will continue to play an important role towards understanding the importance and ecological roles of protists in global geochemical cycling.

    Subscription Required. Please recommend JoVE to your librarian.

    Disclosures

    We have nothing to disclose.

    Acknowledgements

    The authors thank J. Priscu, A. Chiuchiolo and the McMurdo LTER limnology team for assistance in collection and preservation of the samples in Antarctica. We thank Ratheon Polar Services and PHI helicopters for logistical support. Light micrographs were generated in Miami's Center for Advanced Microscopy and Imaging Center. This work was supported by NSF Office of Polar Programs Grants 0631659 and 1056396.

    Materials

    Name Company Catalog Number Comments
    BBM Sigma-Aldrich B5282
    BG11 Sigma-Aldrich C3061
    F/2 Sigma-Aldrich G9903
    GF/F filter, 25 mm Fisher Scientific 09-874-64
    GF/F filter, 47 mm Fisher Scientific 09-874-71
    Polyethersulfone filter, 0.45 μm pore, 47 mm Pall Corporation 61854
    Sterile cell culture flask, 25 cm2 Corning 430639
    Diurnal growth chamber VWR international 35960-076
    Zirconia/silica beads, 0.1 mm diamter Biospec Products 11079101z
    Mini-Bead beater Biospec Products 3110BX
    Screw-cap microcentrifuge tube (1.5 μL) USA Scientific, Inc. 1415-8700
    NaH14CO3 ViTrax VC 194 Keep in aliquots of 400 μL at -20°C
    RuBP Sigma-Aldrich R0878-100mg Dissolve in 10 mM Tris-propionic acid (pH 6.5)

    References

    1. Morgan-Kiss, R. M., Priscu, J. P., Pocock, T., Gudynaite-Savitch, L., Hüner, N. P. A. Adaptation and acclimation of photosynthetic microorganisms to permanently cold environments. Microbiol Mol. Biol. Rev. 70, 222-252 (2006).
    2. Priscu, J. C., Wolf, C. F., Takacs, C. D., Fritsen, C. H., Laybourn-Parry, J., Roberts, J. K. M., Berry-Lyons, W. Carbon transformations in the water column of a perennially ice-covered Antarctic Lake. Biosci. 49, 997-1008 (1999).
    3. Caron, D. A., Worden, A. Z., Countway, P. D., Demir, E., Heidelberg, K. B. Protists are microbes too: a perspective. ISME J. 3, 4-12 (2009).
    4. Bielewicz, S., Bell, E. M., Kong, W., Friedberg, I., Priscu, J. C., Morgan-Kiss, R. M. Protist diversity in a permanently ice-covered Antarctic lake during the polar night transition. ISME J. 5, 1559-1564 (2011).
    5. Laybourn-Parry, J. No place too cold. Science. 324, 1521-1522 (2009).
    6. Roberts, E. C., Laybourn-Parry, J. Mixotrophic cryptophytes and their predators in the Dry Valley lakes of Antarctica. Freshwat. Biol. 41, 737-746 (1999).
    7. Roberts, E. C., Priscu, J. C., Laybourn-Parry, J. Microplankton dynamics in a perennially ice-covered Antarctic lake-Lake Hoare. Freshwat Biol. 27, 238-249 (2004).
    8. Bell, E. M., Laybourn-Parry, J. Mixotrophy in the Antarctic phytoflagellate Pyramimonas gelidicola. J. Phycol. 39, 644-649 (2003).
    9. De Wever, A., Leliaert, F., Verleyen, E., Vanormelingen, P., Van der Gucht, K., Hodgson, D. A. Hidden levels of phylodiversity in Antarctic green algae: further evidence for the existence of glacial refugia. Proc. Biol. Sci. 276-3591 (2009).
    10. Laybourn-Parry, J. Survival mechanisms in Antarctic lakes. Philos. Trans. R. Soc. Lond. B. Biol. Sci. 357, 863-869 (2002).
    11. Lizotte, M. P., Priscu, J. C. Distribution, succession and fate of phytoplankton in the dry valley lakes of Antarctica, based on pigment analysis. Ecosystem Dynamics in a Polar Desert: The McMurdo Dry Valleys. Priscu, J. C. 229-240 (1998).
    12. Ellis, R. J. Most abundance protein in the world. Tren. Biochem. Sci. 4, 241-244 (1979).
    13. Tortell, P. D., Martin, C. L., Corkum, M. E. Inorganic carbon uptake and intracellular assimilation by subarctic Pacific phytoplankton assemblages. Limnol. Oceanogr. 51, 2102-2110 (2006).
    14. Jeffrey, S. W., Humphrey, G. F. New spectrophotometric equations for determining chlorophyll a, b, c1, c2 in higher plants, algae and natural phytoplankton. Biochem. Physiol. Pflanz. 167, 191-194 (1975).
    15. Morgan, R. M., Ivanov, A. G., Priscu, J. C., Maxwell, D. P., Hüner, N. P. A. Structure and composition of the photochemical apparatus of the Antarctic green alga, Chlamydomonas subcaudata. Photosyn. Res. 56, 303-314 (1998).
    16. Guillard, R. R. L. Culture of phytoplankton for feeding marine invertebrates. Culture of Marine Invertebrate Animals. Smith, W. L., Chanley, M. H. Plenum Publishing. New York. 29-60 (1975).
    17. Johnson, M. D., Tengs, T., Oldach, D., Stoecker, D. K. Sequestration, performance, and functional control of cryptophyte plastids in the ciliate Myrionecta rubra (Ciliophora. J. Phycol. 42, 1235-1246 (2006).
    18. Rippka, R., Deruelles, J., Waterbury, J., Herdman, M., Stanier, R. Generic assignments, strain histories and properties of pure cultures of cyanobacteria. J. Gen. Microbiol. 111, 1-61 (1979).
    19. Not, F., del Campo, J., Balague, V., De Vargas, C., Massana, R. New insights into the diversity of marine picoeukaryotes. PLoS ONE. 4, e7143 (2009).
    20. Sherr, B. F., Sherr, E. B., Caron, D. A., Vaulot, D., Worden, A. Z. Oceanic Protists. Oceanography. 20, 130-135 (2007).
    21. Finlay, B. J. Protist taxonomy: an ecological perspective. Philos. Trans. R. Soc. Lond. B. Biol. Sci. 359, 599-610 (2004).
    22. Foissner, W. Protist diversity: estimates of the near-imponderable. Protist. 150, 363-368 (1999).
    23. Gast, R. J., Moran, D. M., Dennett, M. R., Caron, D. A. Kleptoplasty in an Antarctic dinoflagellate: caught in evolutionary transition. Environmental Microbiology. 9, 39-45 (2007).
    24. Gast, R. J., Moran, M. A., Beaudoin, D. J., Blythe, J. N., Dennett, M. R., Caron, D. A. High abundance of a novel dinoflagellate phylotype in the Ross Sea. Antarctica. J. Phycol. 42, 233-242 (2006).
    25. Moran, D. M., Anderson, O. R., Dennett, M. R., Caron, D. A., Gast, R. J. A Description of Seven Antarctic Marine Gymnamoebae Including a New Subspecies, Two New Species and a New Genus: Neoparamoeba aestuarina antarctica n. subsp., Platyamoeba oblongata n. sp., Platyamoeba contorta n. sp. and Vermistella antarctica n. gen. n. sp. Journal of Eukaryotic Microbiology. 54, 169-183 (2007).
    26. Rose, J. M., Vora, N. M., Countway, P. D., Gast, R. J., Caron, D. A. Effects of temperature on growth rate and gross growth efficiency of an Antarctic bacterivorous protist. The ISME journal. 3, 252-260 (2009).

    Comments

    0 Comments

    Post a Question / Comment / Request

    You must be signed in to post a comment. Please or create an account.

    Metrics

    Waiting
    simple hit counter