. 2005 Aug;187(16):5761–5766. doi:10.1128/JB.187.16.5761-5766.2005

The Carbon-Concentrating Mechanism of the Hydrothermal Vent ChemolithoautotrophThiomicrospira crunogena

Kimberly P Dobrinski¹,Dana L Longo¹,Kathleen M Scott^1,^*

¹Biology Department, University of South Florida, Tampa, Florida

Corresponding author. Mailing address: University of South Florida, 4202 East Fowler Avenue, SCA 110, Tampa, FL 33620. Phone: (813) 974-5173. Fax: (813) 974-3263. E-mail:kscott@cas.usf.edu.

Received 2005 Feb 26; Accepted 2005 May 25.

PMC Copyright notice

PMCID: PMC1196061 PMID:16077123

Chemolithoautotrophic bacteria grow in habitats with a variety of dissolved inorganic carbon (DIC) concentrations and are likely to have transport-related adaptations to DIC scarcity. Carbon-concentrating mechanisms (CCMs) are present in many species of cyanobacteria, enabling them to grow in the presence of low concentrations of CO₂ by utilizing bicarbonate transporters and CO₂ traps to generate high intracellular concentrations of DIC. Similar CCMs may also be present in many other autotrophic bacteria. The sulfur-oxidizing γ-proteobacterial chemolithoautotrophThiomicrospira crunogena experiences broad fluctuations in DIC availability at its hydrothermal vent habitat and may use a CCM to facilitate growth during periods of CO₂ scarcity.T. crunogena was cultivated in chemostats under DIC limitation to determine whether it has a CCM. ItsK_DIC for growth was 0.22 mM, with a maximum growth rate of 0.44 h⁻¹. In short-term incubations with [¹⁴C]DIC, DIC-limited cells had higher affinities for DIC (0.026 mM) than DIC-sufficient cells (0.66 mM). DIC-limited cells demonstrated an ability to use both extracellular CO₂ and HCO₃⁻, as assayed by isotopic disequilibrium incubations. These cells also accumulated intracellular DIC to concentrations 100× higher than extracellular, as determined using the silicone oil centrifugation technique. Cells that were not provided with an electron donor did not have elevated intracellular DIC concentrations. The inducible changes in whole-cell affinity for DIC, the ability to use both extracellular CO₂ and HCO₃⁻, and the energy-dependent generation of elevated intracellular concentrations of DIC are all consistent with the presence of a CCM inT. crunogena.

Some 2.7 billion years ago, this planet was geochemically, ecologically, and biologically distinct from what it is today. Atmospheric carbon dioxide concentrations were 1 to 3 orders of magnitude higher (16,30). Representatives from all three domains of life (Archaea,Bacteria, andEukarya) were already present and had begun to diversify (3). Confronted with the precipitous fall of atmospheric and oceanic CO₂ concentrations in the late Proterozoic, many autotrophic lineages likely responded with adaptations to maintain an adequate supply of CO₂ for growth (27,35).

Carbon-concentrating mechanisms (CCMs) can facilitate rapid autotrophic growth in environments where the CO₂ and/or HCO₃⁻ concentrations are chronically or episodically low. CCMs are present in many species of cyanobacteria and generate an elevated intracellular concentration of HCO₃⁻ by using active HCO₃⁻ transport (22,32) and CO₂ traps (33). Carboxysomal carbonic anhydrase (EC 4.2.1.1) converts intracellular HCO₃⁻ to CO₂, which is fixed by ribulose 1,5-bisphosphate carboxylase/oxygenase (Rubisco; EC 4.1.1.39) (2,15,26). The elevated intracellular concentrations of dissolved inorganic carbon (DIC) resulting from active transport expedite carbon fixation by Rubisco by enhancing substrate availability and mitigating the Rubisco oxygenase reaction (15).

CCMs have not been rigorously studied for any other prokaryotic autotrophs (e.g., autotrophicProteobacteria, planktomycetes, green sulfur bacteria,Aquificales, andArchaea). This is surprising, as CCMs are likely to be quite relevant to primary productivity in the diverse habitats where autotrophic microorganisms are found. CCMs with similarities to those present in cyanobacteria may be widespread. For example, the recently sequenced genomes of the photosynthetic α-proteobacteriumRhodopseudomonas palustris and the ammonia-oxidizing β-proteobacteriumNitrosomonas europaea contain genes for carbonic anhydrase and potential HCO₃⁻ transporters (4,18). Furthermore, it has recently been demonstrated that carboxysomes from the chemolithoautotrophHalothiobacillus neapolitanus contain carbonic anhydrase and are believed to function similarly to those present in cyanobacteria (34).

A CCM could facilitate the growth of chemolithoautotrophs at hydrothermal vents, where there is an enormous degree of spatial and temporal variability in the concentration of CO₂ (9). The hydrothermal vent γ-proteobacteriumThiomicrospira crunogena is an obligate sulfur-oxidizing chemoautotroph that was originally isolated from a deep-sea hydrothermal vent habitat where the CO₂ concentration oscillates between 20 μM and 1 mM, and HCO₃⁻ is always the most abundant form of DIC (equal to the sum of CO₂, HCO₃⁻, and CO₃²⁻) (9,11). This is one of the fastest-growing chemoautotrophs, with a doubling time as low as 1 h (11). It continues to grow rapidly in batch culture even after drawing the concentration of DIC down to less than 20 μM, and it has carboxysomes (31). Both characteristics are consistent with the presence of a CCM.

Detailed physiological experiments were undertaken to determine whether this organism has a carbon-concentrating mechanism. Understanding howT. crunogena and other autotrophic microorganisms adapt to low concentrations of DIC during growth is relevant to understanding the physiology of these unique organisms and will provide insights into the response of autotrophic carbon fixation to changes in global geochemistry over Earth history.

MATERIALS AND METHODS

Analytical methods and reagents.

DIC (CO₂ plus HCO₃⁻ plus CO₃²⁻) was quantified with an Agilent 6890N gas chromatograph equipped with an extractor to permit stripping dissolved gases from aqueous samples (5). Ammonia (NH₃ plus NH₄⁺) was assayed using a commercial colorimetric kit (Sigma Inc.). After sonicating the cells for 30 s in the presence of glass beads, total protein was measured with a Lowry-type assay (Bio-Rad Inc.).

The [¹⁴C]DIC used to measure carbon uptake and fixation rates was purchased as a sterile pH 9.5 solution (2 mCi ml⁻¹, 50 mM DIC; MP Biomedicals Inc.). Upon receipt, 0.5-ml portions were sealed into glass vials with gas-tight gas chromatograph septa and stored at 4°C until use. These stock [¹⁴C]DIC solutions had stable counts over the course of this study (unpublished data).

Bacterial strains and growth conditions.

Thiomicrospira crunogena XCL-2 (1) was cultivated at 25°C on liquid and solid TASW media modified from reference11. TASW medium consists of artificial seawater supplemented with 40 mM thiosulfate, whichT. crunogena utilizes as an electron donor, and Na HEPES to maintain the pH at 8 (100 mM in batch culture and 10 mM for continuous culture). The strain was maintained long term in 15% (vol/vol) glycerol-TASW medium at −80°C.

Cultivation under nutrient limitation.

T. crunogena was cultivated in chemostats (New Brunswick Scientific BioFlo 110) to grow the cells under DIC or ammonia limitation. dO₂/pH controllers monitored the pH and O₂ concentrations in the growth chambers with electrodes, maintaining optimal growth conditions by adding 10 N KOH to keep the pH between 7.8 and 8 and by periodically pulsing the growth chamber with O₂ gas to maintain its concentration between 3 and 25 μM. The growth chamber was supplied with TASW medium [2.5 mM DIC, 6.6 mM (NH₄)₂SO₄] from a 10-liter reservoir at a range of dilution rates (0.03 to 0.44 h⁻¹).

Measurement of inducible changes in the half-saturation constant for DIC.

To determine whetherT. crunogena has inducible adaptations to cope with lower concentrations of DIC during growth, DIC-limited and DIC-sufficient (but ammonia limited) cells were cultivated in chemostats at a dilution rate of 0.1 vessel volume h⁻¹ and their whole-cell affinities for DIC were measured. For DIC-sufficient cells, the reservoir [DIC] was raised to 10 mM, and the ammonia concentration was dropped from 13.2 mM to 0.5 mM. When the dilution rate was 0.1 vessel volume h⁻¹, the steady-state [DIC] in the growth chamber was 0.08 mM for DIC-limited cells and 5.5 mM for DIC-sufficient cells. The growth chamber ammonia concentration for DIC-sufficient cells was below the limit of detection for the assay used (<10 μM). DIC or ammonia was confirmed to be limiting growth by observing higher biomass densities in the growth chamber, assayed as protein concentrations, when either DIC or ammonia concentrations (as appropriate) were raised.

To harvest the cells, 150-ml portions were removed from the growth chamber and centrifuged (5,000 ×g, 4°C, 10 min). Pellets were resuspended in 3 ml TASW medium (for DIC-limited cells, trace DIC, 13.2 mM ammonia; for ammonia-limited cells, 5.5 mM DIC and 0.5 mM ammonia) and kept on ice until the experiment was completed (less than 30 min).

Ten-microliter aliquots of the suspended cells were added to seven glass reaction vials with stir bars, filled with 1.98 ml TASW medium (pH 8, 0.02 to 10 mM DIC, supplemented with [¹⁴C]DIC to a specific activity of 2 to 40 Ci/mol). Once per minute, over a time course of 4 min, a 400-μl aliquot was removed from each reaction vial and injected into a scintillation vial containing 200 μl 65°C glacial acetic acid. These acidified samples were gently sparged with air until dry to remove the [¹⁴C]DIC. Scintillation cocktail was added to quantify the organic¹⁴C. Initial activities were measured by injecting 10-μl portions of the incubations into scintillation vials containing 3 ml scintillation cocktail plus 50 μl β-phenethylamine.

Bicarbonate and carbon dioxide uptake and fixation.

To determine whether DIC-limited cells can use both extracellular bicarbonate and carbon dioxide, DIC-limited cells were cultivated and harvested as described above and resuspended in DIC-free TASW medium and bubbled with soda lime-treated (carbon dioxide-free) air until [DIC] = 0. Cell suspensions were then placed on ice and gently sparged with carbon dioxide-free air until use. Incubations with¹⁴C were conducted as described above, with the following modifications. Instead of using [¹⁴C]DIC equilibrated at pH 8, an isotopic disequilibrium technique was used, in which either H¹⁴CO₃⁻ or¹⁴CO₂ was added (6). The¹⁴C stock solution was pH 9.5 in distilled water, and therefore <0.1% CO₂, ∼30% HCO₃⁻, and 70% CO₃²⁻. Upon injection into a well-buffered pH 8 solution, the HCO₃⁻ concentration instantaneously jumps to 93% due to protonation of most of the CO₃²⁻. To prepare dissolved¹⁴CO₂,¹⁴C stock solution was added to DIC-free 1 mM H₃PO₄ in a sealed glass vial and allowed to equilibrate for ∼30 min before use to quantitatively convert the [¹⁴C]DIC to¹⁴CO₂.

Ten-microliter aliquots of suspended cells were added to reaction vials filled with 2 ml DIC-free TASW medium. H¹⁴CO₃⁻ or¹⁴CO₂ was added to the vials to begin the reaction, and time points were taken at 10-s intervals. Upon addition,¹⁴CO₂ generates H¹⁴CO₃⁻ with a half-dehydration time of ∼17 s, while¹⁴CO₂ forms from H¹⁴CO₃⁻ with a half-hydration time of 26 min (37). Accordingly, incubations in which¹⁴CO₂ or H¹⁴CO₃⁻ was initially added were limited to 20 s or 40 s, respectively.

Intracellular DIC accumulation and pH.

The silicone oil centrifugation method was used to measure the size of the intracellular DIC pool and the intracellular pH (modified from reference14). DIC-limited cells were grown and harvested as described above. Eppendorf tubes (0.6 ml) were prepared containing two immiscible layers of fluid: a dense bottom layer, consisting of 20 μl of a killing solution (2:1 [vol/vol] 1 M glycine, pH 10, Triton) overlaid with 65 μl of silicone oil (Dow Chemicals SF 1156). Cell suspensions (200 μl) were pipetted on top of the silicone oil layer, mixed with radiolabeled solute, and, at timed intervals, were centrifuged for 20 s. The cells passed through the silicone layer and pelleted in the killing solution, carrying intracellular radiolabeled solute. Immediately after centrifugation, the tubes were frozen in liquid nitrogen and the bottom layer with the cells was clipped into scintillation vials containing 200 μl glacial acetic acid (for measuring intracellular fixed carbon) or directly into 3 ml scintillation cocktail plus 50 μl β-phenethylamine (for quantifying intracellular fixed and inorganic carbon, cell volumes, or pH).

For measuring intracellular DIC, TASW medium containing 3 to 240 μM [¹⁴C]DIC (40 Ci mol⁻¹) was allowed to equilibrate at pH 8 before the experiment. Two hundred-microliter portions of this solution were pipetted on top of the silicone layers in Eppendorf tubes, and 10 μl of suspended cells in DIC-free TASW medium was added. After 30 s, the tubes were spun at 14,000 ×g for 20 s before freezing and processing, as preliminary time course experiments indicated that the intracellular DIC pool was constant after 20 s. For each concentration of DIC, samples were run in parallel: to measure intracellular DIC plus fixed carbon, pellets were clipped into scintillation cocktail alkalinized with β-phenethylamine to measure fixed carbon, they were clipped into glacial acetic acid. Values from the samples clipped into glacial acetic acid were subtracted from those clipped into alkalinized scintillation cocktail to calculate the intracellular DIC pool. For estimating intracellular volume, which is necessary for calculating intracellular solute concentrations, incubations were also conducted with 9 μCi ml⁻¹d-sorbitol (U-¹⁴C; MP Biomedicals) and 3 μCi ml⁻¹ tritiated water (Amersham Biosciences) (14,29). The intracellular concentrations of both of these substances reached equilibrium before 2 min (unpublished data). Accordingly, incubations with sorbitol or tritium were terminated at 2 min by centrifugation.

To assess whether DIC accumulation was energy dependent or simply driven by intracellular alkalinization, the intracellular pH of DIC-limited cells was measured using the silicone oil centrifugation technique described above, with [¹⁴C]methylamine hydrochloride (ME; MP Biomedicals Inc.). ME has a pK_a of 10.7 and accumulates inside cells as its positively charged, conjugate acid when the cytoplasmic pH is lower than the extracellular pH (29,38). ME was added to cell suspensions (pH 8) to an activity of 0.45 μCi ml⁻¹ and allowed to equilibrate for 3 min, which was sufficient time to reach equilibrium concentrations inside the cells (K. Scott, unpublished data). Parallel incubations with [¹⁴C]sorbitol and tritiated water were conducted with the cell suspensions to make it possible to estimate the intracellular concentrations of the ME.

Due to concern that ME might be accumulating in the cells via uptake by ammonia permeases (20), intracellular pH was also measured with [2-¹⁴C]dimethadione (DMO) (5,5-dimethyl-2,4-oxazolidinedione; American Radiolabeled Chemicals) (29,38). DMO has a pK_a of 6.2 (29,38) and accumulates inside cells as its negatively charged, conjugate base. Incubating cells with DMO under conditions where the extracellular pH is much more alkaline than the intracellular pH prevents DMO from accumulating within the cells. To raise intracellular DMO concentrations, the pH used for incubations with this compound was 7.3 instead of 8.0. A second series of incubations with ME were also conducted at pH 7.3.

Energy dependence of intracellular DIC accumulation.

Cells were cultivated under DIC-limiting conditions as described above. To prepare them for these experiments, it was necessary to wash them four times with thiosulfate-free artificial seawater medium as this electron donor is present in their growth medium at a high concentration (40 mM). After the final wash, cells were resuspended in DIC-free, thiosulfate-free medium and put on ice while being gently bubbled with CO₂-free air. Silicone oil centrifugation experiments with radiolabeled DIC were conducted as described above, at a range of thiosulfate concentrations (0 to 1 mM).

RESULTS

Cultivation under DIC limitation.

Steady-state exponential growth, confirmed by protein and DIC assays, occurred after ∼6 liters of TASW medium had passed through the 1-liter growth chamber. The steady-state DIC concentrations in the growth chamber were substantially lower than in the reservoir due to consumption byT. crunogena (Fig.1). A rectangular hyperbola was fitted to the data via the direct linear plot method (8) to estimate theK_DIC (0.22 mM) and the maximum growth rate (μ_max) (0.44 h⁻¹).

FIG. 1. — Steady-state growth rate constants (μ) and DIC concentrations forT. crunogena cells grown in chemostats under DIC limitation. Using the direct linear plot method (8), a rectangular hyperbola was generated to model the data (shown as a curve in the figure;K_DIC = 0.22 mM; μ_max = 0.44 h⁻¹). The error bars indicate the standard error of the measurements (n = 3).

Measurement of inducible changes in the half-saturation constant for DIC.

DIC-limited cells had much higher whole-cell affinities for DIC (K_DIC = 0.026 mM) than DIC-sufficient cells did (K_DIC = 0.66 mM; Fig.2), which is consistent with inducible changes in transport and/or fixation occurring when cells were growing under DIC-limiting conditions.

Bicarbonate and carbon dioxide uptake and fixation.

T. crunogena demonstrated an ability to use both extracellular carbon dioxide and bicarbonate (Fig.3). Some interconversion of carbon dioxide and bicarbonate did occur over the time course of these experiments and needs to be considered when interpreting the results. When¹⁴CO₂ was initially added, the H¹⁴CO₃⁻ formed was unlikely to contribute substantially to the observed carbon fixation rates, as the initial concentration of CO₂ was low (1 to 6 μM) relative to theK_{HCO_3⁻} (53.6 μM).

For the experiments in which H¹⁴CO₃⁻ was added, the¹⁴CO₂ formed from H¹⁴CO₃⁻ over the 40-s time course probably contributed to the observed carbon fixation rates since the cells demonstrate such a high affinity for CO₂. To account for this, a pseudo-first-order rate constant for CO₂ formation from HCO₃⁻ in seawater was used to calculate the concentration of CO₂ present in the incubations at each time point (37). The contribution of this CO₂ to the measured rates of carbon fixation was estimated using theK_CO₂ (1.03 μM) andV_max (97.2 nmol min⁻¹ mg protein⁻¹) for CO₂-dependent carbon fixation. When this estimate of CO₂-dependent carbon fixation was subtracted from the rates measured in these experiments, theK_{HCO_3⁻} was 11 μM and theV_max was 52 nmol min⁻¹ mg protein⁻¹.

The data are consistent with bicarbonate use contributing substantially to growth under DIC limitation. At pH 8 and 80 μM DIC, the conditions under which these cells were grown, the bicarbonate concentration was 74 μM and the carbon dioxide concentration was ∼0.7 μM (19). Using theK_s andV_max values (Fig.3; parameters for HCO₃⁻ use corrected as described above) and the Michaelis-Menten equation, the carbon fixation rates due to bicarbonate and carbon dioxide use are 45 and 39 nmol min⁻¹ mg protein⁻¹, respectively. Whether DIC-sufficient cells also demonstrate an ability to use extracellular bicarbonate remains to be determined; our manipulations of the DIC concentration in the cell suspensions to prepare them for these experiments would likely induce the expression of the same traits observed in DIC-limited cells.

Intracellular DIC accumulation and pH.

Intracellular concentrations of DIC exceeded the extracellular concentration by 100× (Fig.4), consistent with energy-dependent bicarbonate transport and accumulation in the cytoplasm. The intracellular pH ofT. crunogena is ∼7 at extracellular pHs of 8 (ME, 6.88 ± 0.10) and 7.3 (ME, 7.03 ± 0.06; DMO, 7.01 ± 0.32) (pH ± standard error;n = 3), precluding intracellular alkalinization as the driving force for intracellular DIC accumulation.

Energy dependence of intracellular DIC accumulation.

Cells accumulated elevated intracellular concentrations of DIC when thiosulfate was present at concentrations greater than 1 μM (Fig.5). This correlation of DIC accumulation and thiosulfate presence is consistent with intracellular DIC accumulation relying on either the membrane potential or ATP synthesis resulting from thiosulfate oxidation.

DISCUSSION

T. crunogena has a CCM that enables it to grow in the presence of low concentrations of CO₂ by generating an elevated concentration of intracellular DIC. The results presented here are consistent with active transport of bicarbonate or carbon dioxide playing a role. Active transport could create elevated intracellular DIC concentrations despite the intracellular pH being lower than the extracellular pH and would require the presence of thiosulfate or other electron donors for energy.

A CCM may serve to supplement the supply of CO₂ available atT. crunogena's hydrothermal vent habitat. Temperature differences between bottom water (2°C) and dilute hydrothermal fluid (up to 35°C) create turbulent eddies at the vents. In turn, these eddies are responsible for seconds-to-hours-long oscillations of environmental CO₂ from 1 mM down to ∼20 μM CO₂ (9,12). During the lower-CO₂ periods, a CCM would enableT. crunogena to continue to grow rapidly.

The CCM present inT. crunogena has many parallels with cyanobacterial CCMs. In both cases, whole-cell affinities increase in response to the concentration of DIC available during growth. Energy-dependent transport generates an elevated concentration of intracellular DIC which, presumably inT. crunogena as in cyanobacteria, is “harvested” by carboxysomes (2,26,34). Use of extracellular HCO₃⁻ (Fig.3) is consistent with the presence of HCO₃⁻ transporters, and a high cellular affinity for CO₂ (1 μM) compared to Rubisco (30 to 140 μM for form IA, 100 to 250 μM for form II) (10) may be indicative of an active CO₂ uptake system.

T. crunogena's genome (Scott, unpublished) encodes some genes whose products may function similarly to the components of cyanobacterial CCMs. An α-type carboxysome operon, which includes an ɛ-class carbonic anhydrase gene (34), is present. Additionally, a gene for a SulP-type anion transporter has been found, similar to the SulP-type transporters from marine cyanobacteria that have recently been demonstrated to have HCO₃⁻-transporting activity (24).

It is also likely that theT. crunogena CCM will have several features that distinguish it from cyanobacterial CCMs. In contrast to cyanobacteria, whose genomes have a single form IA or form IB Rubisco gene (13,21,23,28),T. crunogena's genome carries three genes for this enzyme (two form IA Rubisco genes and one form II Rubisco gene). The two form I Rubisco genes are expressed when cells are grown under low DIC conditions, while the form II Rubisco gene is preferentially expressed under high DIC conditions (Scott, unpublished), similar to what has been observed forHydrogenovibrio marinus (36). Also different from cyanobacteria,T. crunogena's genome lacks any apparent homologs for the cyanobacterial bicarbonate transporter genescmpABCD (22) andsbtA (32), as well aschpX andchpY, which encode key components of the cyanobacterial CO₂ uptake system (25,33). It is possible that novel HCO₃⁻ and CO₂ transporters will be found in this organism, and it will be interesting to determine whether transporter and Rubisco gene expression is coordinately regulated. The generation of random and directed knockout mutants is under way (K. P. Dobrinski and K. M. Scott, unpublished data), with the objective of deciphering the mechanism for intracellular DIC accumulation in this organism.

T. crunogena is not likely to be the only chemolithoautotroph with a CCM. CCMs may be present in other chemolithoautotrophs that have a high demand for DIC (e.g., due to rapid growth rates), utilize a sufficiently abundant or electronegative electron donor to offset the energetic burden of a CCM, and inhabit an environment with periods of DIC or CO₂ scarcity. Mechanistic and genetic studies of CCMs in several lineages ofBacteria andArchaea have the potential to illuminate how their ancestors coped with the 2-order-of-magnitude drop in CO₂ availability occurring over Earth history (16,30).

Autotrophs may have addressed this dilemma with a single solution that was spread by horizontal gene transfer (as Rubisco genes were) (7). Alternatively, each lineage may have come up with a unique solution. It is reasonable to anticipate lineage-specific innovation, based on cyanobacterial CCMs. In cyanobacteria, three nonhomologous bicarbonate-transporting systems and two forms of carboxysomes are scattered among the different clades (2,24). Other autotrophs inhabit microhabitats even more disparate than those where cyanobacteria flourish (17) and embrace an astounding degree of phylogenetic and physiological diversity (at least four divisions ofBacteria andArchaea). Perhaps this ecological and phylogenetic diversity is reflected in a genetic and mechanistic diversity of CCMs.

Acknowledgments

Thanks are due to Douglas Nelson for providing the strain ofT. crunogena used for this study; to Gordon Cannon for illuminating discussions; to Stacy Guerin and Darinka Obradovich for expert assistance with the experiments; to Peter Girguis, Shana Goffredi, and Zoe McCudden for editing early versions of the manuscript; and to two anonymous reviewers for helpful suggestions.

This work was supported in part by a New Researcher grant (USF).

REFERENCES

1.Ahmad, A., J. P. Barry, and D. C. Nelson. 1999. Phylogenetic affinity of a wide, vacuolate, nitrate-accumulatingBeggiatoa sp. from Monterey Canyon, California, withThioploca spp. Appl. Environ. Microbiol. 65:270-277. [DOI] [PMC free article] [PubMed] [Google Scholar]
2.Badger, M., D. Hanson, and G. D. Price. 2002. Evolution and diversity of CO₂ concentrating mechanisms in cyanobacteria. Funct. Plant Biol. 29:161-173. [DOI] [PubMed] [Google Scholar]
3.Brocks, J. J., G. A. Logan, R. Buick, and R. E. Summons. 1999. Archean molecular fossils and the early rise of eukaryotes. Science 285:1033-1036. [DOI] [PubMed] [Google Scholar]
4.Chain, P., J. Lamerdin, F. Larimer, W. Regala, V. Lao, M. Land, L. Hauser, A. Hooper, M. Klotz, J. Norton, L. Sayavedra-Soto, D. Arciero, N. Hommes, M. Whittaker, and D. Arp. 2003. Complete genome sequence of the ammonia-oxidizing bacterium and obligate chemolithoautotrophNitrosomonas europaea. J. Bacteriol. 185:2759-2773. [DOI] [PMC free article] [PubMed] [Google Scholar]
5.Childress, J. J. 1984. Metabolic and blood characteristics in the hydrothermal vent tube-wormRiftia pachyptila. Mar. Biol. 83:109-124. [Google Scholar]
6.Cooper, T. G., and D. Filmer. 1969. The active species of “CO₂” utilized by ribulose diphosphate carboxylase. J. Biol. Chem. 244:1081-1083. [PubMed] [Google Scholar]
7.Delwiche, C. F., and J. D. Palmer. 1996. Rampant horizontal transfer and duplication of rubisco genes in eubacteria and plastids. Mol. Biol. 13:873-882. [DOI] [PubMed] [Google Scholar]
8.Eisenthal, R., and A. Cornish-Bowden. 1974. The direct linear plot. Biochem. J. 139:715-720. [DOI] [PMC free article] [PubMed] [Google Scholar]
9.Goffredi, S. K., J. J. Childress, N. T. Desaulniers, R. W. Lee, F. H. Lallier, and D. Hammond. 1997. Inorganic carbon acquisition by the hydrothermal vent tubewormRiftia pachyptila depends upon high external P-CO₂ and upon proton-equivalent ion transport by the worm. J. Exp. Biol. 200:883-896. [DOI] [PubMed] [Google Scholar]
10.Horken, K., and F. R. Tabita. 1999. Closely related form I ribulose bisphosphate carboxylase/oxygenase molecules that possess different CO₂/O₂ substrate specificities. Arch. Biochem. Biophys. 361:183-194. [DOI] [PubMed] [Google Scholar]
11.Jannasch, H. W., C. O. Wirsen, D. C. Nelson, and L. A. Robertson. 1985.Thiomicrospira crunogena sp. nov., a colorless, sulfur-oxidizing bacterium from a deep-sea hydrothermal vent. Int. J. Syst. Bacteriol. 35:422-424. [Google Scholar]
12.Johnson, K. S., J. J. Childress, and C. L. Beehler. 1988. Short term temperature variability in the Rose Garden hydrothermal vent field. Deep-Sea Res. 35:1711-1722. [Google Scholar]
13.Kaneko, T., Y. Nakamura, C. P. Wolk, T. Kuritz, S. Sasamoto, A. Watanabe, M. Iriguchi, A. Ishikawa, K. Kawashima, T. Kimura, Y. Kishida, M. Kohara, M. Matsumoto, A. Matsuno, A. Muraki, N. Nakazaki, S. Shimpo, M. Sugimoto, M. Takazawa, M. Yamada, M. Yasuda, and S. Tabata. 2001. Complete genomic sequence of the filamentous nitrogen-fixing cyanobacterium Anabaena sp. strain PCC 7120. DNA Res. 8:205-213. [DOI] [PubMed] [Google Scholar]
14.Kaplan, A., M. R. Badger, and J. A. Berry. 1980. Photosynthesis and the intracellular inorganic carbon pool in the bluegreen algaAnabaena variabilis: response to external CO₂ concentration. Planta 149:219-226. [DOI] [PubMed] [Google Scholar]
15.Kaplan, A., R. Schwarz, J. Lieman-Hurwitz, M. Ronen-Tarazi, and L. Reinhold. 1994. Physiological and molecular studies on the response of cyanobacteria to changes in the ambient inorganic carbon concentration, p. 469-485.In D. A. Bryant (ed.), The molecular biology of cyanobacteria. Kluwer Academic Publishers, Dordrecht, The Netherlands.
16.Kaufman, A. J., and S. Xiao. 2003. High CO₂ levels in the Proterozoic atmosphere estimated from analyses of individual microfossils. Nature 425:279-282. [DOI] [PubMed] [Google Scholar]
17.Kuenen, J. G., and P. Bos. 1989. Habitats and ecological niches of chemolitho(auto)trophic bacteria, p. 117-146.In H. G. Schlegel and B. Bowien (ed.), Autotrophic bacteria. Springer-Verlag, Madison, Wis.
18.Larimer, F., P. Chain, L. Hauser, J. Lamerdin, S. Malfatti, L. Do, M. Land, D. Pelletier, J. Beatty, A. Lang, F. R. Tabita, J. L. Gibson, T. Hanson, C. Bobst, J. T. Y. Torres, C. Peres, F. Harrison, J. Gibson, and C. Harwood. 2004. Complete genome sequence of the metabolically versatile photosynthetic bacteriumRhodopseudomonas palustris. Nat. Biotechnol. 22:55-61. [DOI] [PubMed] [Google Scholar]
19.Lewis, E., and D. W. R. Wallace. 1998. Program developed for CO₂ system calculations, ORNL/CDIAC-105. Oak Ridge National Laboratory, U.S. Department of Energy, Oak Ridge, Tenn.
20.Muro-Pastor, M., J. C. Reyes, and F. J. Florencio. 2005. Ammonium assimilation in cyanobacteria. Photosynth. Res. 83:135-150. [DOI] [PubMed] [Google Scholar]
21.Nakamura, Y., T. Kaneko, S. Sato, M. Mimuro, H. Miyashita, T. Tsuchiya, S. Sasamoto, A. Watanabe, K. Kawashima, Y. Kishida, C. Kiyokawa, M. Kohara, M. Matsumoto, A. Matsuno, N. Nakazaki, S. Shimpo, C. Takeuchi, M. Yamada, and S. Tabata. 2003. Complete genome structure of Gloeobacter violaceus PCC 7421, a cyanobacterium that lacks thylakoids. DNA Res. 10:137-145. [DOI] [PubMed] [Google Scholar]
22.Omata, T., G. D. Price, M. R. Badger, M. Okamura, S. Gohta, and T. Ogawa. 1999. Identification of an ATP-binding cassette transporter involved in bicarbonate uptake in the cyanobacteriumSynechococcus sp. strain PCC 7942. Proc. Natl. Acad. Sci. USA 96:13571-13576. [DOI] [PMC free article] [PubMed] [Google Scholar]
23.Palenik, B., B. Brahamsha, F. W. Larimer, M. Land, L. Hauser, P. Chain, J. Lamerdin, W. Regala, E. Allen, J. McCarren, I. Paulsen, A. Dufresne, F. Partensky, E. Webb, and J. Waterbury. 2003. The genome of a motile marineSynechococcus. Nature 424:1037-1042. [DOI] [PubMed] [Google Scholar]
24.Price, G., F. Woodger, M. Badger, S. Howitt, and L. Tucker. 2004. Identification of a SulP-type bicarbonate transporter in marine cyanobacteria. Proc. Natl. Acad. Sci. USA 101:18228-18233. [DOI] [PMC free article] [PubMed] [Google Scholar]
25.Price, G. D., S. Maeda, T. Omata, and M. R. Badger. 2002. Modes of active inorganic carbon uptake in the cyanobacterium, Synechococcus sp. PCC7942. Funct. Plant Biol. 29:131-149. [DOI] [PubMed] [Google Scholar]
26.Price, G. D., D. Sultemeyer, B. Klughammer, M. Ludwig, and M. Badger. 1998. The functioning of the CO₂ concentrating mechanism in several cyanobacterial strains: a review of general physiological characteristics, genes, proteins, and recent advances. Can. J. Bot. 76:973-1002. [Google Scholar]
27.Raven, J. A. 1991. Implications of inorganic carbon utilization: ecology, evolution, and geochemistry. Can. J. Bot. 69:908-923. [Google Scholar]
28.Rocap, G., F. W. Larimer, J. Lamerdin, S. Malfatti, P. Chain, N. A. Ahlgren, A. Arellano, M. Coleman, L. Hauser, W. R. Hess, Z. I. Johnson, M. Land, D. Lindell, A. F. Post, W. Regala, M. Shah, S. L. Shaw, C. Steglich, M. B. Sullivan, C. S. Ting, A. Tolonen, E. A. Webb, E. R. Zinser, and S. W. Chisholm. 2003. Genome divergence in two Prochlorococcus ecotypes reflects oceanic niche differentiation. Nature 424:1042-1047. [DOI] [PubMed] [Google Scholar]
29.Rottenberg, H. 1979. The measurement of membrane potential and ΔpH in cells, organelles, and vesicles. Methods Enzymol. 55:547-569. [DOI] [PubMed] [Google Scholar]
30.Rye, R., P. H. Kuo, and H. D. Holland. 1995. Atmospheric carbon dioxide concentrations before 2.2 billion years ago. Nature 378:603-605. [DOI] [PubMed] [Google Scholar]
31.Scott, K. M., M. Bright, and C. R. Fisher. 1998. The burden of independence: inorganic carbon utilization strategies of the sulphur chemoautotrophic hydrothermal vent isolateThiomicrospira crunogena and the symbionts of hydrothermal vent and cold seep vestimentiferans. Cah. Biol. Mar. 39:379-381. [Google Scholar]
32.Shibata, M., H. Katoh, M. Sonoda, H. Ohkawa, M. Shimoyama, H. Fukuzawa, A. Kaplan, and T. Ogawa. 2002. Genes essential to sodium-dependent bicarbonate transport in cyanobacteria. J. Biol. Chem. 277:18658-18664. [DOI] [PubMed] [Google Scholar]
33.Shibata, M., H. Ohkawa, H. Katoh, M. Shimoyama, and T. Ogawa. 2002. Two CO₂ uptake systems in cyanobacteria: four systems for inorganic carbon acquisition inSynechocystis sp. strain PCC6803. Funct. Plant Biol. 29:123-129. [DOI] [PubMed] [Google Scholar]
34.So, A. K.-C., G. S. Espie, E. B. Williams, J. M. Shively, S. Heinhorst, and G. C. Cannon. 2004. A novel evolutionary lineage of carbonic anhydrase (ɛ class) is a component of the carboxysome shell. J. Bacteriol. 186:623-630. [DOI] [PMC free article] [PubMed] [Google Scholar]
35.Tortell, P. D. 2000. Evolutionary and ecological perspectives on carbon acquisition in phytoplankton. Limnol. Oceanogr. 45:744-750. [Google Scholar]
36.Yoshizawa, Y., K. Toyoda, H. Arai, M. Ishii, and Y. Igarashi. 2004. CO₂-responsive expression and gene organization of three ribulose-1,5-bisphosphate carboxylase/oxygenase enzymes and carboxysomes inHydrogenovibrio marinus strain MH-110. J. Bacteriol. 186:5685-5691. [DOI] [PMC free article] [PubMed] [Google Scholar]
37.Zeebe, R. E., and D. Wolf-Gladrow. 2003. CO₂ in seawater: equilibrium, kinetics, isotopes. Elsevier, New York, N.Y.
38.Zilberstein, D., V. Agmon, S. Schuldiner, and E. Padan. 1984.Escherichia coli intracellular pH, membrane potential, and cell growth. J. Bacteriol. 158:246-252. [DOI] [PMC free article] [PubMed] [Google Scholar]

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The Carbon-Concentrating Mechanism of the Hydrothermal Vent ChemolithoautotrophThiomicrospira crunogena

Kimberly P Dobrinski

Dana L Longo

Kathleen M Scott