Energy metabolism of Heliobacterium modesticaldum during phototrophic and chemotrophic growth
© Tang et al; licensee BioMed Central Ltd. 2010
Received: 4 March 2010
Accepted: 24 May 2010
Published: 24 May 2010
Heliobacterium modesticaldum is a gram-positive nitrogen-fixing phototrophic bacterium that can grow either photoheterotrophically or chemotrophically but not photoautotrophically. Surprisingly, this organism is lacking only one gene for the complete reverse tricarboxylic acid (rTCA) cycle required for autotrophic carbon fixation. Along with the genomic information reported recently, we use multiple experimental approaches in this report to address questions regarding energy metabolic pathways in darkness, CO2 fixation, sugar assimilation and acetate metabolism.
We present the first experimental evidence that D-ribose, D-fructose and D-glucose can be photoassimilated by H. modesticaldum as sole carbon sources in newly developed defined growth medium. Also, we confirm two non-autotrophic CO2-fixation pathways utilized by H. modesticaldum: reactions catalyzed by pyruvate:ferredoxin oxidoreductase and phosphoenolpyruvate carboxykinase, and report acetate excretion during phototrophic and chemotrophic growth. Further, genes responsible for pyruvate fermentation, which provides reducing power for nitrogen assimilation, carbon metabolism and hydrogen production, are either active or up-regulated during chemotrophic growth. The discovery of ferredoxin-NADP+ oxidoreductase (FNR) activity in cell extracts provides the reducing power required for carbon and nitrogen metabolisms. Moreover, we show that photosynthetic pigments are produced by H. modesticaldum during the chemotrophic growth, and demonstrate that H. modesticaldum performs nitrogen fixation during both phototrophic and chemotrophic growth.
Collectively, this report represents the first comprehensive studies for energy metabolism in heliobacteria, which have the simplest known photosynthetic machinery among the entire photosynthetic organisms. Additionally, our studies provide new and essential insights, as well as broaden current knowledge, on the energy metabolism of the thermophilic phototrophic bacterium H. modesticaldum during phototrophic and chemotrophic growth.
Several features characterize the physiological and metabolic aspects of phototrophic heliobacteria [1–5]: (a) They are the only known phototrophs that belong to the gram-positive bacterial phylum Firmicutes, and as is typical of members of this group, which includes species of Bacillus and Clostridium, heliobacteria can form heat resistant endospores; (b) They produce the unique pigment bacteriochlorophyll g (BChl g); (c) They produce 81-hydroxy-chlorophyll a with a farnesol tail (81-OH-Chl aF), which serves as the primary electron acceptor from the reaction center (RC) special pair; (d) They contain a type I homodimeric RC bound to the cytoplasmic membrane; (e) They require organic carbon sources for both phototrophic growth and chemotrophic (fermentative) growth; and (f) they are active nitrogen-fixers and also produce hydrogen. Further, Heliobacterium modesticaldum, isolated from hot springs microbial mats and volcanic soils in Iceland , is one of only two known anoxygenic phototrophs that can fix nitrogen at temperatures higher than 50°C (the other is Chlorobaculum tepidum) [7, 8].
Genomic sequence data of H. modesticaldum suggests that several genes required for the known autotrophic carbon fixation pathways are missing . This is consistent with previous physiological studies indicating that heliobacteriaceae are obligate heterotrophs . In the absence of known CO2-fixation mechanisms, it is unknown whether alternative pathways may be adapted by H. modesticaldum for CO2 assimilation. The genomic information suggests that one candidate for anaplerotic CO2 incorporation is phosphoenolpyruvate (PEP) carboxykinase. We recently identified the non-autotrophic, anaplerotic CO2 assimilation mechanism in the photoheterotrophic α-proteobacterium Roseobacter denitrificans . Whether a similar anaplerotic pathway and/or other pathways are employed for CO2 incorporation in H. modesticaldum has not been verified.
It has been reported that pyruvate, lactate, acetate, and yeast extract can support photoheterotrophic growth of H. modesticaldum [2, 6]. Although essential genes in the oxidative pentose phosphate (PP) and Entner-Doudoroff (ED) pathways are absent in the genome, genes for the Embden-Meyerhof-Parnas (EMP) pathway (glycolysis), gluconeogenesis, and a ribose ATP-binding cassette (ABC) transporter (rbsABCD) have been annotated in the genome. However, neither hexose nor ribose has been reported to support the growth of H. modesticaldum . Additionally, while the most vigorous growth of H. modesticaldum occurs photoheterotrophically, H. modesticaldum can also grow chemotrophically (dark, anoxic) by fermentation . But heliobacterial energy metabolism during chemotrophic (fermentative) growth is not fully understood. To address these questions about the carbon and energy metabolism of H. modesticaldum, experimental evidence gathered using a multi-faceted approach and working hypotheses are presented in this report.
D-ribose, D-fructose and D-glucose can support the growth of H. modesticaldum
By optimizing the growth conditions, we successfully grew the cultures on D-ribose, D-glucose and D-fructose in the growth medium containing 0.02% yeast extract (i.e. "vitamin level" yeast extract), whereas no growth can be detected with only 0.02% yeast extract in the culture medium (Figure 1A). Cell growth is dependent on the concentration of D-sugars, and no growth of H. modesticaldum is seen with 40 mM 2'-fluoro-2'-deoxy-D-glucose (FDG) as the sole carbon source (Figure 1B). Lack of the growth on FDG, a glucose analogue, is consistent with the mechanism of action of FDG that cannot be metabolized inside the cells because it lacks the 2'-hydroxyl group in normal glucose required for conversion of D-glucose-6-phosphate to D-fructose-6-phosphate in glycolysis. Alternatively, no growth is detected on L-arabinose, which is one of the most abundant pentoses present as a constituent of bacterial cell wall and is a more common isomer than D-arabinose. Many bacteria contain an inducible operon that encodes a series of enzymes and transporters that allows L-arabinose to be used as a sole carbon source in cell culture. No arabinose transporter (araE) is annotated in the genome of H. modesticaldum.
In addition to physiological studies, we also determine the uptake of D-hexose and assay the enzymatic activity for the enzymes specific for the EMP pathway. Our studies indicate 20-25% D-fructose (8-10 mM) and ~10% D-glucose (~4 mM) being assimilated, consistent with better growth on D-fructose than on D-glucose. No acetate is excreted from 40 mM glucose-grown cultures (data not shown). Enzymatic activity of hexokinase (10 nmole/min•mg protein), 6-phosphofructokinase (20 nmole/min•mg protein) and pyruvate kinase (10 nmole/min•mg protein), three enzymes specific for the EMP pathway and not shared with the gluconeogenesis pathway, can be detected in hexose-grown cultures. Together, our studies indicate that H. modesticaldum uses the EMP pathway for carbohydrate metabolism when D-glucose, D-fructose and D-ribose are supplied as carbon sources.
Probe glucose photoassimilation by mass spectrometry
As described above, glucose and fructose can enhance the growth of H. modesticaldum in YE medium (Additional file 1: Figure S1). We have investigated the roles of glucose in the cultures grown on glucose and 0.4% yeast extract. In addition to the experimental evidence presented above, we determined the molecular mass of photosynthetic pigments of H. modesticaldum, BChl g and 81-OH-Chl aF (BChl g, 819 Da; 81-OH-Chl aF, 835 Da), in glucose-grown cultures by MALDI-TOF mass spectrometry. If glucose is photo-assimilated via the EMP pathway to produce cell materials of H. modesticaldum, BChl g and 81-OH-Chl aF should be labeled when 13C-labeled glucose (Glc) is added to the growth medium. To test the hypothesis, we obtain mass spectra of (B)Chls extracted from pyruvate-grown cultures as the positive control, since pyruvate has been established as the sole carbon source for H. modesticaldum. (B)Chls were extracted as reported previously . Because an acidic matrix (α-cyano-4-hydroxycinnamic acid) was used to prepare the samples submitted to mass spectral analysis, peaks corresponding to demetallization of BChl g and 81-OH-Chl aF were detected (upon demetallization (M-22; - Mg2+ + 2 H+): BChl g, 797 Da; 81-OH-Chl aF, 813 Da) (Figure 1C, upper panel, and Figure 1D, upper panel). Compared to the sample from unlabeled pyruvate-grown cultures (Figure 1C, upper panel), higher molecular masses corresponding to labeled (B)Chls (BChl g, 817 Da; 81-OH-Chl aF, 833 Da) were detected using [3-13C]pyruvate as the sole carbon source (Figure 1C, lower panel).
Growth on yeast extract
As previously reported , we also found that yeast extract (0.4%) alone can support growth of H. modesticaldum (Figure 2A). It is known that many undefined carbon sources, vitamin mixtures and amino acids included, are included in yeast extract. We successfully replaced yeast extract with vitamin B12 for supporting the growth of a different photoheterotrophic bacterium . In all of the growth media of H. modesticaldum, vitamin B12 has always been included, and it is not yet known what carbon sources in the yeast extract support the photoheterotrophic growth of H. modesticaldum. With approaches listed in Materials and Methods, we have estimated that the amount of pyruvate, acetate and lactate in yeast extract is negligible. However, the inclusion of pyruvate or acetate as a defined organic carbon source, along with yeast extract, can significantly enhance growth (Additional file 2: Figure S2). Alternatively, it is possible that some amino acids in yeast extract may support the growth of H. modesticaldum, and the oxidation of amino acids transported into the cell can generate reducing power and chemical energy. To test this hypothesis, we grew H. modesticaldum on casamino acids that contain predominately a mixture of free amino acids, and observed comparable cell growth with 1.0% casamino acids versus with 0.4% yeast extract after 48 hours of growth (OD625 is ~0.7-0.8). Also, we didn't observe significant growth enhancement with vitamin mixtures included in casamino acids-grown cultures. Together, our studies support the idea that amino acids contribute to the growth of H. modesticaldum. Further, we have probed the contribution of glutamate and glutamine for cell growth of H. modesticaldum. Glutamate can serve as a nitrogen source for H. modesticaldum , while our current studies indicate that either glutamate or glutamine (up to 100 mM each) cannot support the growth of H. modesticaldum as a sole carbon source during phototrophic and chemotrophic growth.
Organic carbon sources used in growth media reported in this paper.
pyruvate-mineral salt medium
pyruvate (20 mM)
pyruvate-yeast extract medium
pyruvate (phototrophic growth, 20 mM; chemotrophic growth, 40 mM), yeast extract (0.4%)
yeast extract medium
yeast extract (0.4%)
acetate-mineral salt medium
acetate (40 mM), HCO3- (20 mM)
 and this report
hexose- and ribose-grown medium
sugar (hexose or ribose, 40 mM), yeast extract (0.02%)
 and this report
Non-autotrophic CO2 assimilation by H. modesticaldum
It has been recognized that pyruvate is the preferred organic carbon source for heliobacteria and it can support both photoheterotrophic and chemotrophic growth . Consistent with previous reports, our studies show that H. modesticaldum grows better using pyruvate as carbon source compared to other organic carbon sources (Figure 2A), and the rate of cell growth corresponds to that of pyruvate consumption (Figure 2B). In contrast to CO2-enhanced growth of Chlorobaculum (Cba.) tepidum and other green sulfur bacteria , no difference in growth rate can be detected with or without 0.4% HCO3- included in pyruvate-grown cultures (Figure 2B). Moreover, no growth can be detected with HCO3- as the sole carbon source (Figure 2A).
The lack of autotrophic growth in H. modesticaldum can be attributed to the lack of a gene encoding ATP citrate lyase (ACL) [1, 5], which catalyzes the cleavage of citrate to acetyl-CoA and oxaloacetate (OAA) and is one of the key enzymes specific in the autotrophic CO2 fixation via the reductive (or reverse) tricarboxylic acid (rTCA) cycle [13–15]. To confirm the absence of an enzyme having ACL activity, we performed activity assays in cell-free extracts of H. modesticaldum and Cba. tepidum. The latter served as a positive control for ACL activity, which is documented in Cba. tepidum [16, 17]. Consistent with previous reports, the activity of ACL was clearly detected in cell free extracts of Cba. tepidum, but not in H. modesticaldum (Additional file 4: Figure S3). Additionally, the activity of citrate synthase, catalyzing the formation of citrate from condensation of OAA and acetyl-CoA in the oxidative TCA cycle, also cannot be detected (data not shown).
Gene expression profiles for phototrophic (light) vs. chemotrophic (dark) growth.
Relative gene expression level (light/dark)c
Genes for carbon metabolism
15.0 ± 0.1
22.0 ± 0.1
7.0 ± 0.2
pykA (pyruvate kinase)
13.5 ± 0.1
19.5 ± 0.1
6.0 ± 0.2
porA (pyruvate:Fd oxidoreductase)
13.7 ± 0.1
11.6 ± 0.0
-2.1 ± 0.1
fdxR (Fd-NADP+ oxidoreductase)
14.7 ± 0.1
15.2 ± 0.1
0.5 ± 0.2
13.4 ± 0.1
13.2 ± 0.1
-0.2 ± 0.2
14.0 ± 0.1
14.3 ± 0.1
0.3 ± 0.2
ackA (acetate kinase)
10.6 ± 0.1
12.2 ± 0.1
1.6 ± 0.2
acsA (acetyl-CoA synthase)
15.5 ± 0.1
21.0 ± 0.1
5.5 ± 0.2
ppdK (pyruvate phosphate dikinase)
13.4 ± 0.1
17.4 ± 0.1
4.0 ± 0.2
pckA (PEP carboxykinase)
14.1 ± 0.1
17.2 ± 0.1
3.1 ± 0.2
mdh (malate dehydrogenase)
14.5 ± 0.1
14.6 ± 0.1
0.1 ± 0.2
Genes for pigment biosynthesis
13.1 ± 0.1
15.7 ± 0.0
2.6 ± 0.1
14.0 ± 0.0
18.0 ± 0.1
4.0 ± 0.1
13.2 ± 0.1
15.0 ± 0.1
1.8 ± 0.2
12.9 ± 0.1
13.9 ± 0.1
1.0 ± 0.2
Genes for nitrogen assimilation and hydrogen production
nifK (Fe/Mo nitrogenase, β subunit)
13.0 ± 0.0
21.5 ± 0.1
8.5 ± 0.1
nifD (Fe/Mo nitrogenase, α subunit)
13.7 ± 0.0
21.4 ± 0.1
7.7 ± 0.1
hupS ([NiFe]-hydrogenase small subunit)
13.3 ± 0.1
18.4 ± 0.1
5.1 ± 0.2
hupL ([NiFe]-hydrogenase large subunit)
12.7 ± 0.1
18.3 ± 0.1
5.6 ± 0.2
hymD (Fe only hydrogenase, Hymd subunit)
13.4 ± 0.1
18.7 ± 0.1
5.3 ± 0.2
14.3 ± 0.2
19.7 ± 0.1
5.4 ± 0.3
12.9 ± 0.2
18.6 ± 0.1
5.7 ± 0.3
12.9 ± 0.1
18.6 ± 0.1
5.7 ± 0.2
Acetate can serve as a carbon source with CO2-enhanced growth
where Fdred and Fdox represent the reduced and oxidized form of ferredoxin (Fd), respectively.
The porA gene (HM1_0807), encoding PFOR, has been annotated in H. modesticaldum. The enzymatic activity of PFOR has been reported in pyruvate-grown cultures of Heliobacterium strain HY-3 . In some relatives of the heliobacteria, such as Clostridium thermoaceticum and other clostridia, PFOR is linked to the carbon fixation via the reductive acetyl-CoA pathway (i.e. the Wood-Ljungdahl pathway) . While enzymes that function in this autotrophic carbon fixation pathway are commonly found in both methanogens and acetate-producing clostridia , they are not found in the genome of H. modesticaldum .
Phototrophic versus chemotrophic growth of H. modesticaldum
(A) Acetate assimilation and excretion
Nutrient uptake and metabolite excretion in PMS medium (pyruvate as the sole carbon source) during various growth conditions.
Pyruvate supplied/consumed (mM)
Acetate excretion (mM)
Ratio of pyruvate consumption/acetate excretion
Lactate excretion (mM)
phototrophic growth + 0.4% bicarbonate
While our results are different from the report of Heliobacterium strain HY-3 , the authors found more acetate being produced during chemotrophic growth (13.6 mM) than during phototrophic growth (5.9 mM). Both our and their studies demonstrate that acetate can be produced from pyruvate-grown heliobacterial cultures during phototrophic and chemotrophic growth. Two acetate assimilation/excretion pathways are possibly employed by H. modesticaldum. One is catalyzed by acetyl-CoA synthetase (ACS, EC 188.8.131.52), proceeding through an acetyl adenylate intermediate; and the other is catalyzed by acetate kinase (ACK, EC 184.108.40.206, acetate ⇌ acetyl-phosphate) and phosphotransacetylase (PTA, EC 220.127.116.11, acetyl-phosphate ⇌ acetyl-CoA) . No ACS activity was reported in the studies of Heliobacterium strain HY-3 , and it is possible that ACK and PTA are responsible in the acetate assimilation/excretion pathway in Heliobacterium strain HY-3.
Enzyme activity of enzymes and relative expression level of genes for acetate metabolism in pyruvate-grown cultures during phototrophic and chemotrophic growth.
Specific activity (nmole/min/mg protein)
Enzyme activity tested
Relative gene expression level (light/dark)
acetyl-CoA synthetase (ACS) a
100 ± 20
acetate kinase (ACK) a
800 ± 40
600 ± 100
phosphotransacetylase (PTA) a
400 ± 50
500 ± 100
(B) Gene expression in carbon, nitrogen and hydrogen metabolism
To extend our understanding from the physiological studies shown in Figure 3, we monitored some key genes for carbon, nitrogen and hydrogen metabolism during phototrophic and chemotrophic growth. Compared to the photoheterotrophic growth of H. modesticaldum, in which energy is generated from light and reducing powers (NAD(P)H and Fdred) are generated from light and oxidation of organic carbon (i.e. pyruvate oxidation), less energy and reducing powers are expected to be generated for H. modesticaldum in darkness. In agreement with this hypothesis, most of the genes involved in energy metabolism are down-regulated during chemotrophic growth (Table 2 and Figure 4). For instance, genes encoding enzymes for (1) the EMP pathway (pfkA (HM1_0078), 6-phosphofructokinase, and pykA (HM1_0076), pyruvate kinase); (2) nitrogen assimilation (nifD (HM1_0864) and nifK (HM1_0865), subunits of molybdenum-dependent group I type (FeMo-co) nitrogenase); and (3) hydrogen production (hupS (HM1_1478) and hupL (HM1_1479), subunits of uptake nickel-iron ([NiFe])-hydrogenase (hupSL); nuoEFG (HM1_1028 - HM1_1029), encoding [FeFe]-hydrogenase; and hymD (HM1_1590), encoding the Hymd subunit of Fe-only dehydrogenase).
(C) Pyruvate metabolism is either active or up-regulated in darkness
Note that high FNR activity (10 μmole/min•mg protein) is detected in the cell free extract of H. modesticaldum (Additional file 5: Figure S4). Consistent with the studies of FNR from other organisms, we also detected that FNR in H. modesticaldum has higher specificity for NADPH versus NADH, and that the reaction turnover for producing Fdred, by measuring the formation of NADP+ or NAD+ (equation 2), is more than 50-fold faster for NADPH than for NADH (Additional file 5: Figure S4A). The rate of NADPH oxidation is accelerated with addition of ferricyanide (Additional file 5: Figure S4B). Together, the discovery of FNR activity in cell extracts indicates that the reducing power required for carbon and nitrogen metabolisms in H. modesticaldum can be generated from FNR during phototrophic and chemotrophic growth.
(D) Photosynthetic pigments produced in darkness
(E) Nitrogen is assimilated during phototrophic and chemotrophic growth
Biological nitrogen assimilation (i.e. diazotrophic growth) is an ancient process that is widely distributed in prokaryotes, and is found in some members of all groups of phototrophic bacteria . Previous studies showed that nitrogen assimilation in heliobacterial cultures is "switched-off" when NH4+ is supplied as the nitrogen source and activated with N2(g) supplied [6, 24], and that H. modesticaldum is one of the only two known anaerobic anoxygenic phototrophs that can fix nitrogen at temperatures above 50°C [6, 7]. Significant amounts of chemical energy (16 ATP) and reducing power (8 Fdred) are required during diazotrophic growth (N2 + 8 H+ + 8 Fdred + 16 ATP → 2 NH3 + H2 + 8 Fdox + 16 ADP + 16 Pi) .
D-sugars are photoassimilated by H. modesticaldum
While the EMP pathway is annotated in the genome, no sugar-supported growth has been reported for H. modesticaldum. It is not uncommon for microorganisms that have the EMP pathway annotated but do not use glucose and other sugars as carbon sources, and to date only one heliobacterium, Heliobacterium gestii, has been reported to grow on C6-sugars, i.e. glucose and fructose . Alternatively, fermentation of glucose through the EMP pathway has been reported in non-phototrophic bacteria in the phylum Firmicutes [26, 27]. In this paper, we present the first report on the growth of H. modesticaldum supported by D-ribose, D-glucose and D-fructose with "vitamin-level" (0.02%) yeast extract included. With the support of multiple lines of experimental evidence, including physiological studies, activity assays, gene expression data, and mass spectra, our work addresses the puzzle that the EMP pathway has previously been annotated but no sugar-supported growth has been reported for H. modesticaldum.
The growth on D-ribose confirms the proposed function of a putative ribose ABC transporter (rbsDACB, HM1_2417 - HM1_2420) and ribokinase (rbsK, HM1_2416) through genome annotation, and growth supported by D-ribose, D-glucose and D-fructose suggests that annotated EMP and non-oxidative pentose phosphate pathways in H. modesticaldum are active in carbohydrate metabolism. As D-fructose and D-glucose are polar molecules, glucose, fructose or hexose transporter proteins are required to move those molecules across the cell membrane into the cells. No known hexose transporter has been reported for H. modesticaldum, which may partially explain slower growth on D-hexose than on D-ribose. It remains to be determined if the putative ribose transporter of H. modesticaldum functions as a hexose transporter, since no ribose transporter has been reported previously to accommodate a hexose.
Metabolism of carbohydrate through the EMP pathway supplies 2 ATP and 2 NADH to the cells, which are significant for the energy metabolism of H. modesticaldum, because essential genes in the oxidative pentose phosphate and ED pathways, which provide reducing equivalents during carbohydrate metabolism, are absent in the genome. Moreover, utilization of glucose can provide an additional path for H2 production in H. modesticaldum as reported in some non-phototrophic bacteria .
The biological significance of the alternative CO2-assimilation pathways
The CO2-anaplerotic pathways are known to replenish the intermediates of TCA cycle, so that removal of the intermediates for synthesizing cell materials will not significantly slow down the metabolic flux through the TCA cycle. Our recent studies showed that the photoheterotrophic bacterium R. denitrificans uses the anaplerotic pathways to assimilate CO2. All of the genes encoding the enzymes for CO2-anaplerotic pathways, PEP carboxylase, PEP carboxykinase, pyruvate carboxylase and malic enzyme, have been annotated in the R. denitrificans genome, and activities of these enzymes have been detected. The alternative CO2-fixation pathways account for making up 10-15% cellular proteins of R. denitrificans . Our studies presented here also suggest that H. modesticaldum uses two anaplerotic pathway, PEP carboxykinase (PEPCK) and pyruvate:ferredoxin oxidoreductase (PFOR), for assimilating CO2.
What is the biological importance of PEPCK and PFOR in H. modesticaldum? Although the anaplerotic CO2-assimilation cannot support (photo)heterotrophic growth in the way that the autotrophic CO2-fixation supports (photo)autotrophs, these two CO2-anaplerotic pathways are critical for the carbon metabolism of H. modesticaldum (see Figure 5). First, the CO2-assimilation by PFOR catalyzes the formation of pyruvate from acetyl-CoA, a reaction that cannot be catalyzed by pyruvate dehydrogenase. Hence, PFOR is essential for acetate assimilation and pyruvate metabolism. Second, as shown in Figure 5, PEPCK is required to convert PEP into OAA in the partial reductive TCA (rTCA) cycle. Without assimilating CO2 by PEPCK, carbon flux through the partial rTCA cycle cannot take place.
Possible functions of PFOR and FNR during chemotrophic growth
H. modesticaldum is one of the only two cultured anoxygenic phototrophs that can fix nitrogen at temperatures above 50°C. Only acetate, lactate and pyruvate have been reported previously to support the photoheterotrophic growth of H. modesticaldum, and it is necessary to further explore carbon sources in order to understand energy metabolism in-depth. In this paper, we developed the growth medium close to a minimal growth medium, and report the first studies, with comprehensive experimental evidence supported, that D-ribose, D-glucose and D-fructose can be photoassimilated as sole carbon sources to generate cell material. Additionally, in the absence of autotrophic CO2 fixation, H. modesticaldum uses two CO2-anaplerotic pathways during phototrophic growth: pyruvate:ferredoxin oxidoreductase (PFOR) and phosphoenol-pyruvate carboxykinase (PEPCK). The CO2-anaplerotic pathways by PFOR and PEPCK are essential for acetate assimilation, pyruvate metabolism and introducing carbon flow into the rTCA cycle for generating cell materials, including photosynthetic pigments (Figure 5).
Our studies suggest that PFOR and ferredoxin-NADP+ oxidoreductase (FNR) are required for generating reducing power (Fdred and NAD(P)H) during chemotrophic growth. A similar ratio of acetate excretion/pyruvate consumption is observed in pyruvate-grown cultures during phototrophic versus chemotrophic growth, and conversion of acetyl-CoA to acetate can generate ATP for the energy required for H. modesticaldum in darkness. Also, since energy and reducing power produced by H. modesticaldum during chemotrophic growth are rather limited compared to phototrophic growth, cellular functions demanding high-energy input, such as nitrogen fixation and hydrogen production, are down-regulated. Nevertheless, our studies indicate that H. modesticaldum produces sufficient energy and reducing power for both carbon metabolism and nitrogen fixation during chemotrophic growth, albeit at a relatively low growth rate. An overview of energy metabolism pathways of H. modesticaldum is shown in Figure 8. In summary, our reported studies not only significantly broaden our current knowledge, but also provide new and essential insights on the energy metabolism of H. modesticaldum.
Chemicals and enzymes for enzymatic activity assays were purchased from Sigma-Aldrich. The 13C-labeled glucose and pyruvate were from Cambridge Isotope Laboratories (CIL), Inc. The DNA oligomers were from Integrated DNA Technology (IDT) without further purification. The source culture of Heliobacterium modesticaldum Ice1T was a gift from the laboratory of Dr. Michael T. Madigan at Southern Illinois University, Carbondale.
The growth of bacterial strains
All Heliobacterium modesticaldum Ice1T cultures reported in this work were grown anaerobically inside a Coy anaerobic chamber at temperatures ranging from 46-50°C, and cell growth was estimated turbidimetrically at OD625. OD625 was chosen for evaluating the cell growth because absorbance of photosynthetic pigments is minimal around 625 nm (as shown in Figure 6). Phototrophic cultures were grown in low-intensity light (10 ± 1 W/m2), and chemotrophic cultures were grown in darkness. The list of growth media used in this report and organic carbon sources included in each medium are described in Table 1. The pyruvate mineral salts (PMS, with 20 mM (2.2 g/L) pyruvate included) medium were prepared as reported previously . The chemicals in yeast extract (YE) medium (per liter) are: K2HPO4 (1.0 g), MgSO4•7H2O (0.2 g), CaCl2•2H2O (20 mg), Na2S2O3•5H2O (0.2 g), yeast extract (4.0 g), (NH4)2SO4 (1.0 g), chelated iron solution  (2 ml), d-biotin (15 μg), vitamin B12 (20 μg) and trace element solution (1 ml) with the final pH adjusted to pH 6.9-7.0. Components of the trace element solution were reported previously . Pyruvate (20 mM for phototrophic growth and 40 mM for chemotrophic growth) is added to YE medium to prepare pyruvate-yeast extract (PYE) medium. Sodium acetate (40 mM) and HCO3- (20 mM) are included in acetate-mineral salts (AMS) medium, and sugar (hexose or ribose) (40 mM) and "vitamin level" yeast extract (0.02%) are included in sugar-grown medium. Cultures of H. modesticaldum were grown either photoheterotrophically in PMS, YE, PYE, AMS and different sugar-grown medium (listed in Table 1) or chemotrophically (dark, anoxic) in PYE medium. NH4Cl (in mineral salts medium), (NH4)2SO4 (in YE and PYE medium), and N2/H2 = 98/2 (under nitrogen fixation conditions) was used as the nitrogen source. Typically, 1-2% cultures (50-100 fold dilution) in the late exponential growth phase were used to inoculate fresh media.
Measurement of the uptake of pyruvate, acetate, lactate, fructose and glucose
The amount of pyruvate and lactate in the cultures of H. modesticaldum under different growth conditions was determined by the methods reported previously [9, 29]. The amount of D-glucose and pyruvate in the cultures of H. modesticaldum under different growth conditions was determined by the methods reported previously . Uptake of D-fructose was estimated by a coupled hexokinase/phosphoglucose isomerase/glucose-6-phosphate dehydrogenase assay, and the amount of NADPH formed in the reaction, measured by the increase of the absorbance at 340 nm, is stoichiometric to the amount of D-fructose in solution. The amount of acetate production was determined by a coupled acetyl-CoA synthase/citrate synthase/malate dehydrogenase assay following the formation of NADH .
RNA extraction and quantitative real-time PCR (QRT-PCR)
The methods used to extract RNA and perform QRT-PCR were described previously [9, 31]. QRT-PCR was performed to profile the gene expression under different growth conditions of H. modesticaldum. The primers for QRT-PCR in this report are listed in Additional file 6: Table S2. Two biological replicates, with three technical replicates for each biological sample, were performed for validation, and the mean value was reported. The amplified DNA fragments were verified by 1% agarose gel electrophoresis, and a single fragment was obtained for all amplicons.
Photosynthetic pigments in H. modesticaldum cultures were extracted as reported previously . The mass spectra of the photosynthetic pigments, BChl g and 81-OH-Chl aF, were acquired using matrix-assisted laser desorption ionization-time-of-flight (MALDI-TOF) mass spectrometry. Sample measurements and preparation were described previously .
Cell scattering subtraction of the absorption spectrum
The light scattering of cells was digitally subtracted from the raw data of Figure 6 using the approach described as follows. The scattering presented in the raw data of the original spectrum was first mimicked by an analytical function, , in which a, b, c are variable coefficients and λ is wavelength (nm). An initial function was applied in the long wavelength range, where the pigments absorption does not contribute to the scattering. The fitting equation has been written and applied in Origin 7.5 (Origin Lab Corp.). After obtaining the formula, a scattering simulation was extrapolated to the short wavelength range and subtracted from the original spectrum.
Enzymatic activities were performed with cell-free crude extracts prepared as follows: Cells were harvested by centrifugation at 5,000 × g for 15 min at 4°C and washed with 20 mM Tris-HCl buffer at pH 8.0. The cell pellet was resuspended in the same buffer containing 1 mM phenylmethanesulfonyl fluoride (PMSF). Resuspended cells were disrupted by sonication, and cell debris was removed with centrifugation at 20,000 × g for 30 min. Protein concentration in cell extracts was determined by the Bradford assay  using bovine serum albumin as a standard. The enzymatic activity of acetyl-CoA synthetase, acetate kinase, ATP citrate lyase, citrate synthase, ferredoxin-NADP+ oxidoreductase, hexokinase, phosphenolpyruvate carboxykinase, 6-phosphofructokinase, pyruvate kinase and phosphotransacetylase in cell-free extracts was assayed as described previously [16, 18, 33–39].
The authors thank Dr. W. Matthew Sattley for useful comments on the manuscript, Dr. Dariusz Niedzwiedzki for his help in preparing Figure 6 in this article, and Mr. Jianzhong Wen for his help with the mass spectrometry. This work was supported by a grant from the Exobiology program of NASA to R. E. Blankenship.
- Sattley WM, Madigan MT, Swingley WD, Cheung PC, Clocksin KM, Conrad AL, Dejesa LC, Honchak BM, Jung DO, Karbach LE, Kurdoglu A, Lahiri S, Mastrian SD, Page LE, Taylor HL, Wang ZT, Raymond J, Chen M, Blankenship RE, Touchman JW: The genome of Heliobacterium modesticaldum, a phototrophic representative of the Firmicutes containing the simplest photosynthetic apparatus. J Bacteriol. 2008, 190: 4687-4696. 10.1128/JB.00299-08.PubMed CentralView ArticlePubMedGoogle Scholar
- Madigan MT: The family Heliobacteriaceae. The Prokaryotes. 2006, 4: 951-964. full_text.View ArticleGoogle Scholar
- Madigan MT: Heliobacteriaceae. Bergey's manual of systematic bacteriology. Edited by: Boone DR, Castenholtz RW, Garrity GM. 2001, Springer-Verlag, New York, 1: 625-30. 2View ArticleGoogle Scholar
- Heinnickel M, Golbeck JH: Heliobacterial photosynthesis. Photosynth Res. 2007, 92: 35-53. 10.1007/s11120-007-9162-4.View ArticlePubMedGoogle Scholar
- Sattley WM, Blankenship RE: Insights into heliobacterial photosynthesis and physiology from the genome of Heliobacterium modesticaldum. Photosynth Res.Google Scholar
- Kimble LK, Mandelco L, Woese CR, Madigan MT: Heliobacterium modesticaldum, sp. nov., a thermophilic heliobacterium of hot springs and volcanic soils. Arch Microbiol. 1995, 163: 259-267. 10.1007/BF00393378.View ArticleGoogle Scholar
- Madigan MT: Microbiology of nitrogen fixation by anoxygenic photosynthetic bacteria. Anoxygenic Photosynthetic Bacteria. Edited by: Blankenship RE, Madigan MT, Bauer CE. 1995, Kluwer Academic Publishers, Dordrecht, The Netherlands, 915-928.Google Scholar
- Wahlund TM, Madigan MT: Nitrogen fixation by the thermophilic green sulfur bacterium Chlorobium tepidum. J Bacteriol. 1993, 175: 474-478.PubMed CentralPubMedGoogle Scholar
- Tang KH, Feng X, Tang YJ, Blankenship RE: Carbohydrate metabolism and carbon fixation in Roseobacter denitrificans OCh114. PLoS One. 2009, 4: e7233-10.1371/journal.pone.0007233.PubMed CentralView ArticlePubMedGoogle Scholar
- Michalski TJ, Hunt JE, Bowman MK, Smith U, Bardeen K, Gest H, Norris JR, Katz JJ: Bacteriopheophytin g: Properties and some speculations on a possible primary role for bacteriochlorophylls b and g in the biosynthesis of chlorophylls. Proc Natl Acad Sci USA. 1987, 84: 2570-2574. 10.1073/pnas.84.9.2570.PubMed CentralView ArticlePubMedGoogle Scholar
- Dong MQ, Venable JD, Au N, Xu T, Park SK, Cociorva D, Johnson JR, Dillin A, Yates JR: Quantitative mass spectrometry identifies insulin signaling targets in C. elegans. Science. 2007, 317: 660-663. 10.1126/science.1139952.View ArticlePubMedGoogle Scholar
- Overmann J: The family Chlorobiaceae. The Prokaryotes. 2006, 7: 359-378. full_text.View ArticleGoogle Scholar
- Evans MC, Buchanan BB, Arnon DI: New cyclic process for carbon assimilation by a photosynthetic bacterium. Science. 1966, 152: 673-10.1126/science.152.3722.673-b.View ArticlePubMedGoogle Scholar
- Hugler M, Huber H, Molyneaux SJ, Vetriani C, Sievert SM: Autotrophic CO2 fixation via the reductive tricarboxylic acid cycle in different lineages within the phylum Aquificae: evidence for two ways of citrate cleavage. Environ Microbiol. 2007, 9: 81-92. 10.1111/j.1462-2920.2006.01118.x.View ArticlePubMedGoogle Scholar
- Schmitz RA, Daniel R, Deppenmeier U, Gottschalk G: The anaerobic way of life. The Prokaryotes. 2006, 2: 86-101. full_text.View ArticleGoogle Scholar
- Kim W, Tabita FR: Both subunits of ATP-citrate lyase from Chlorobium tepidum contribute to catalytic activity. J Bacteriol. 2006, 188: 6544-6552. 10.1128/JB.00523-06.PubMed CentralView ArticlePubMedGoogle Scholar
- Wahlund TM, Tabita FR: The reductive tricarboxylic acid cycle of carbon dioxide assimilation: initial studies and purification of ATP-citrate lyase from the green sulfur bacterium Chlorobium tepidum. J Bacteriol. 1997, 179: 4859-4867.PubMed CentralPubMedGoogle Scholar
- Pickett MW, Williamson MP, Kelly DJ: An enzyme and 13C-NMR of carbon metabolism in heliobacteria. Photosynth Res. 1994, 41: 75-88. 10.1007/BF02184147.View ArticlePubMedGoogle Scholar
- Furdui C, Ragsdale SW: The role of pyruvate ferredoxin oxidoreductase in pyruvate synthesis during autotrophic growth by the Wood-Ljungdahl pathway. J Biol Chem. 2000, 275: 28494-28499. 10.1074/jbc.M003291200.View ArticlePubMedGoogle Scholar
- Thauer RK: Microbiology. A fifth pathway of carbon fixation. Science. 2007, 318: 1732-1733. 10.1126/science.1152209.View ArticlePubMedGoogle Scholar
- Kimble LK, Stevenson AK, Madigan MT: Chemotrophic growth of heliobacteria in darkness. FEMS Microbiol Lett. 1994, 115: 51-55. 10.1111/j.1574-6968.1994.tb06613.x.View ArticlePubMedGoogle Scholar
- Castano-Cerezo S, Pastor JM, Renilla S, Bernal V, Iborra JL, Canovas M: An insight into the role of phosphotransacetylase (pta) and the acetate/acetyl-CoA node in Escherichia coli. Microb Cell Fact. 2009, 8: 54-10.1186/1475-2859-8-54.PubMed CentralView ArticlePubMedGoogle Scholar
- Raymond J, Siefert JL, Staples CR, Blankenship RE: The natural history of nitrogen fixation. Mol Biol Evol. 2004, 21: 541-554. 10.1093/molbev/msh047.View ArticlePubMedGoogle Scholar
- Kimble LK, Madigan MT: Nitrogen fixation and nitrogen metabolism in heliobacteria. Arch Microbiol. 1992, 158: 155-161. 10.1007/BF00290810.View ArticleGoogle Scholar
- Howard JB, Rees DC: Structural Basis of Biological Nitrogen Fixation. Chem Rev. 1996, 96: 2965-2982. 10.1021/cr9500545.View ArticlePubMedGoogle Scholar
- Fuhrer T, Fischer E, Sauer U: Experimental identification and quantification of glucose metabolism in seven bacterial species. J Bacteriol. 2005, 187: 1581-1590. 10.1128/JB.187.5.1581-1590.2005.PubMed CentralView ArticlePubMedGoogle Scholar
- Mahowald MA, Rey FE, Seedorf H, Turnbaugh PJ, Fulton RS, Wollam A, Shah N, Wang C, Magrini V, Wilson RK, Cantarel BL, Coutinho PM, Henrissat B, Crock LW, Russell A, Verberkmoes NC, Hettich RL, Gordon JI: Characterizing a model human gut microbiota composed of members of its two dominant bacterial phyla. Proc Natl Acad Sci USA. 2009, 106: 5859-5864. 10.1073/pnas.0901529106.PubMed CentralView ArticlePubMedGoogle Scholar
- de Vrije T, Mars AE, Budde MA, Lai MH, Dijkema C, de Waard P, Claassen PA: Glycolytic pathway and hydrogen yield studies of the extreme thermophile Caldicellulosiruptor saccharolyticus. Appl Microbiol Biotechnol. 2007, 74: 1358-1367. 10.1007/s00253-006-0783-x.View ArticlePubMedGoogle Scholar
- Howell BF, McCune S, Schaffer R: Lactate-to-pyruvate or pyruvate-to-lactate assay for lactate dehydrogenase: a re-examination. Clin Chem. 1979, 25: 269-272.PubMedGoogle Scholar
- Ma K, Hutchins A, Sung SJ, Adams MW: Pyruvate ferredoxin oxidoreductase from the hyperthermophilic archaeon, Pyrococcus furiosus, functions as a CoA-dependent pyruvate decarboxylase. Proc Natl Acad Sci USA. 1997, 94: 9608-9613. 10.1073/pnas.94.18.9608.PubMed CentralView ArticlePubMedGoogle Scholar
- Tang KH, Wen J, Li X, Blankenship RE: Role of the AcsF protein in Chloroflexus aurantiacus. J Bacteriol. 2009, 191: 3580-3587. 10.1128/JB.00110-09.PubMed CentralView ArticlePubMedGoogle Scholar
- Bradford MM: A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem. 1976, 72: 248-254. 10.1016/0003-2697(76)90527-3.View ArticlePubMedGoogle Scholar
- Ainsworth S, MacFarlane N: A kinetic study of rabbit muscle pyruvate kinase. Biochem J. 1973, 131: 223-236.PubMed CentralView ArticlePubMedGoogle Scholar
- Cassan N, Lagoutte B, Setif P: Ferredoxin-NADP+ reductase. Kinetics of electron transfer, transient intermediates, and catalytic activities studied by flash-absorption spectroscopy with isolated photosystem I and ferredoxin. J Biol Chem. 2005, 280: 25960-25972. 10.1074/jbc.M503742200.View ArticlePubMedGoogle Scholar
- Chen ZH, Walker RP, Tecsi LI, Lea PJ, Leegood RC: Phosphoenolpyruvate carboxykinase in cucumber plants is increased both by ammonium and by acidification, and is present in the phloem. Planta. 2004, 219: 48-58. 10.1007/s00425-004-1220-y.View ArticlePubMedGoogle Scholar
- Van Schaftingen E, Jett MF, Hue L, Hers HG: Control of liver 6-phosphofructokinase by fructose 2,6-bisphosphate and other effectors. Proc Natl Acad Sci USA. 1981, 78: 3483-3486. 10.1073/pnas.78.6.3483.PubMed CentralView ArticlePubMedGoogle Scholar
- Gerber G, Preissler H, Heinrich R, Rapoport SM: Hexokinase of human erythrocytes. Purification, kinetic model and its application to the conditions in the cell. Eur J Biochem. 1974, 45: 39-52. 10.1111/j.1432-1033.1974.tb03527.x.View ArticlePubMedGoogle Scholar
- Kumari S, Tishel R, Eisenbach M, Wolfe AJ: Cloning, characterization, and functional expression of acs, the gene which encodes acetyl coenzyme A synthetase in Escherichia coli. J Bacteriol. 1995, 177: 2878-2886.PubMed CentralPubMedGoogle Scholar
- Kuang Y, Salem N, Wang F, Schomisch SJ, Chandramouli V, Lee Z: A colorimetric assay method to measure acetyl-CoA synthetase activity: application to woodchuck model of hepatitis virus-induced hepatocellular carcinoma. J Biochem Biophys Methods. 2007, 70: 649-655. 10.1016/j.jbbm.2007.02.008.PubMed CentralView ArticlePubMedGoogle Scholar
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