- Open Access
Effect of tungstate on acetate and ethanol production by the electrosynthetic bacterium Sporomusa ovata
Biotechnology for Biofuelsvolume 9, Article number: 163 (2016)
Microbial electrosynthesis (MES) and gas fermentation are bioenergy technologies in which a microbial catalyst reduces CO2 into organic carbon molecules with electrons from the cathode of a bioelectrochemical system or from gases such as H2. The acetogen Sporomusa ovata has the capacity of reducing CO2 into commodity chemicals by both gas fermentation and MES. Acetate is often the only product generated by S. ovata during autotrophic growth.
In this study, trace elements in S. ovata growth medium were optimized to improve MES and gas fermentation productivity. Augmenting tungstate concentration resulted in a 2.9-fold increase in ethanol production by S. ovata during H2:CO2-dependent growth. It also promoted electrosynthesis of ethanol in a S. ovata-driven MES reactor and increased acetate production 4.4-fold compared to unmodified medium. Furthermore, fatty acids propionate and butyrate were successfully converted to their corresponding alcohols 1-propanol and 1-butanol by S. ovata during gas fermentation. Increasing tungstate concentration enhanced conversion efficiency for both propionate and butyrate. Gene expression analysis suggested that tungsten-containing aldehyde ferredoxin oxidoreductases (AORs) and a tungsten-containing formate dehydrogenase (FDH) were involved in the improved biosynthesis of acetate, ethanol, 1-propanol, and 1-butanol. AORs and FDH contribute to the fatty acids re-assimilation pathway and the Wood–Ljungdahl pathway, respectively.
This study presented here shows that optimization of microbial catalyst growth medium can improve productivity and lead to the biosynthesis of different products by gas fermentation and MES. It also provides insights on the metabolism of biofuels production in acetogens and demonstrates that S. ovata has an important untapped metabolic potential for the production of other chemicals than acetate via CO2-converting bioprocesses including MES.
Acetogens are anaerobic bacteria capable of growing autotrophically by conducting gas fermentation with H2:CO2 as well as with synthesis gas (H2:CO:CO2) . Another promising feature of acetogens is the ability of some to accept electrons from the cathode of a bioelectrochemical system (BES) to reduce CO2 into multicarbon compounds in a process named microbial electrosynthesis (MES) [2–4]. Gas fermentation is a promising bioproduction process for recycling industrial gas wastes into commodity chemicals, thus limiting greenhouse gas emissions . MES has additional attractive features. It can be used to store electricity surplus from the power grid into the chemical bonds of valuable products like biofuels . It can also be coupled with solar panels to become an artificial bioinorganic photosynthesis apparatus with a solar-to-chemicals conversion efficiency significantly higher than biomass-based bioproduction technologies . Under autotrophic growth conditions, including gas fermentation and MES, acetogens utilize the acetyl-CoA/Wood–Ljungdahl pathway (WL) to reduce CO2 to acetyl-CoA, a precursor in the synthesis of cellular components as well as in the generation of organic carbon products such as acetate and ethanol [1, 6, 7].
One successful approach to improve the production of organic carbon molecules from CO2 by acetogens consists of optimizing the cultivation medium composition [8–10]. For example, ethanol production by the acetogen Clostridium ragsdalei was improved up to fivefold by optimizing traces elements concentration in the growth medium . This approach also led to increase in bacterial growth and acetate production.
Trace elements are mainly required by bacteria because of their role as cofactors for enzymes involved in metabolic pathways such as the WL pathway. In acetogens, key metalloenzymes of the WL pathway include hydrogenases, the formate dehydrogenase (FDH) and the bifunctional CO dehydrogenase (CODH)/acetyl-CoA synthase (ACS) . Hydrogenases perform the reversible oxidation of molecular H2 and require iron only or both iron and nickel [11, 13]. FDHs catalyze the reversible conversion of CO2 to formate . They contain tungsten, iron, selenium, and/or molybdenum, depending on the bacterial species and on the availability of these elements in the growth medium [15, 16]. CODH/ACS is a bifunctional enzyme containing nickel and iron catalyzing the reversible reduction of CO2 to CO and the synthesis of acetyl-CoA [12, 17, 18].
Acetogens producing or oxidizing the solvent ethanol possess other important metalloenzymes including alcohol dehydrogenases (ADH) catalyzing the reversible oxidation of alcohols and requiring zinc or iron for their activity [19, 20]. Due to energetic considerations, ethanol production by acetogens is thought to occur via acetate re-assimilation . In addition to ADH, this pathway also requires a tungsten-containing aldehyde ferredoxin oxidoreductase (AOR) catalyzing the reduction of acetate to acetaldehyde with ferredoxin as the low-potential electron donor [22–24].
A promising platform for the production of multicarbon compounds from CO2 is the Gram-negative bacterium Sporomusa ovata, one of the most efficient acetogenic MES microbial catalysts for the production of acetate reported until now [4, 25, 26]. In this study, we attempted to develop the biosynthesis of ethanol by S. ovata and to improve acetate production rate by optimizing trace elements in the cultivation medium. Production of acetate and ethanol from CO2 with H2 or a cathode as the electron source as well as growth under autotrophic condition was investigated with different concentrations of trace elements (WO4 2−, MoO4 2−, SeO4 2−, Ni2+, Zn2+, and Fe2+) in the medium. Furthermore, transcript abundance of genes coding for critical metalloenzymes involved in the WL pathway or in the synthesis of ethanol like AORs was studied to understand better the molecular mechanisms responsible for the improved growth and productivity caused by changes in trace elements concentration. The conversion of longer carbon chain fatty acids than acetate to alcohols during gas fermentation was also investigated to determine if S. ovata has the metabolic capacity to synthesize longer alcohols than ethanol.
Results and discussion
Impact of varying trace elements concentration on acetate and ethanol production by S. ovata
Optimization of the concentration of different trace elements was investigated with S. ovata under H2:CO2 growth condition. Among all the tested elements (WO4 2−, MoO4 2−, SeO4 2−, Ni2+, Zn2+, and Fe2+), only augmentation of tungstate (WO4 2−) concentration had a significant impact on acetate and ethanol production by S. ovata after 8 days of growth (Fig. 1). The absence of statistically significant changes in acetate and ethanol production in the presence of augmented concentrations of MoO4 2−, SeO4 2−, Ni2+, Zn2+, or Fe2+ indicates that these elements are already present in sufficient concentrations in the standard 311 medium for S. ovata.
Multiplying tungstate concentration by 10 to 0.1 μM in S. ovata 311 growth medium resulted in a 3.1-fold increase in ethanol production compared to standard 311 medium (1× tungstate) and a 8.6-fold increase versus 311 medium without added tungstate (0×) (Fig. 1a). These results indicate that optimal ethanol production by S. ovata is dependent on tungstate concentration. In contrast, acetate production in the presence of 10× tungstate was reduced by 12.0 ± 9.1 % versus standard medium and 17.3 ± 5.4 % compared to medium with 0× tungstate (Fig. 1a), which indicates that part of the acetate may have been re-assimilated by S. ovata to produce ethanol.
Impact of tungstate on autotrophic growth and production of ethanol and acetate by S. ovata
The effect of varying tungstate concentration on growth as well as on ethanol and acetate production was further investigated via H2:CO2 time course experiments over a period of 15 days. Compared to standard medium, omitting tungstate resulted in longer doubling time and lower final OD545, while multiplying tungstate concentration by 10 accelerated growth and increased final OD545 by ca. 1.2-fold (Fig. 2a; Table 1). Ethanol production was increased when tungstate concentration was augmented from 0 to 1× to 5× to 10×. Higher tungstate augmentation to 50× and 100× did not have further impact on ethanol production (Table 1).
As indicated by Fig. 2b, acetate production by S. ovata is growth-dependent. In contrast, ethanol production started at the end of the exponential phase and continued through the stationary phase (Fig. 2b). A pH drop from initial 7.3 to 4.8 was also observed coinciding with the production shift from acetate to ethanol (Fig. 2a). This production shift by S. ovata as well as the pH change in the medium followed the same trend described for other bacterial species including acetogens [10, 27]. In those bacteria, fatty acids (e.g., acetate) are produced first during an acidogenic phase, and solvents (e.g., ethanol) are generated in a second phase termed solventogenic phase when cell growth decreases and the pH become more acid .
Furthermore, the important increase in ethanol especially in the presence of 10× tungstate was accompanied with a notable decrease of acetate (Figs. 1a and 2b). This suggests the production of ethanol by S. ovata via acetate re-assimilation. For instance, the model solvent-producing bacterium Clostridum acetobutylicum can produce the solvents acetone, ethanol, and 1-butanol by re-assimilating fatty acids acetate and butyrate generated in the acidogenic phase, which resulted in an observable concentrations decrease in these fatty acids [28, 29]. A similar phenomenon was also observed for the acetogens C. ragsdalei and C. ljungdahlii during syngas fermentation where ethanol production probably occurs via acetate reduction .
Acetate and ethanol production by MES with optimized medium
One of the most promising applications of S. ovata as a microbial catalyst is the reduction of CO2 into organic carbon products with electrons derived from the cathode of a MES system . Thus, the impact of increasing tungstate concentration on acetate and ethanol production by S. ovata-driven MES was investigated (Fig. 3). A steady consumption of current over time with the concomitant production of acetate and ethanol was observed with 10× tungstate (Fig. 3a). The MES production of acetate was increased 4.4-fold from 32.0 ± 1.7 to 141.2 ± 56.6 mmol m−2 day−1 (380.0 ± 20.0–1694.5 ± 678.6 μM day−1) with 10× tungstate compared to 1× tungstate. These results show that increasing tungstate concentration improves acetate production from CO2 by MES, which may be caused by higher enzymatic capacity in the WL pathway for reactions like the conversion of CO2 to formate by tungsten-containing FDH. As expected, no acetate or ethanol was produced with a disconnected MES reactor control with 10× tungstate over a period of 15 days confirming that the metabolism of S. ovata was driven by current consumption.
1.5 ± 0.5 mM (n = 3) of ethanol was produced during the MES process when tungstate concentration was decupled with a production rate of 4.0 ± 1.2 mmol m−2 day−1 (48.0 ± 14.6 μM day−1) from day 1 to 4 (Fig. 3a). When unmodified 311 medium was used as the electrolyte, no ethanol production by MES was detected (Fig. 3b). To the best of our knowledge, production of ethanol by a pure culture-driven MES system has never been reported until now. Electron recovery in both acetate and ethanol with 10× tungstate was 87.6 ± 6.5 %. However, ethanol did not continue to accumulate over time in the MES system and started to decrease after day 4 (Fig. 3a). There are two possibilities to explain the concentration fluctuation observed with ethanol in S. ovata-driven MES system. First, ethanol could be abiotically lost mainly via evaporation from the MES system. Ethanol is a solvent and the MES reactor used in this study is an open system with constant N2:CO2 gas flushing in the liquid phase. Second, ethanol was biologically reoxidized by S. ovata. To evaluate abiotic loss of ethanol from the MES reactor, a control experiment was set up and 10 mM of ethanol was added to sterile 311 medium in the cathodic chamber with continuous input of N2:CO2 gas mixture over 7 days. Under these conditions, ca. 40 % of ethanol was lost. This observation suggests that the real ethanol production rate from day 1 to 4 in our MES system is underestimated. It may also explain in part why ethanol disappeared after day 4. These results do not exclude the second possibility that S. ovata could reoxidize the produced ethanol. This would be in accordance with the fact that S. ovata can grow with ethanol as sole substrate and that its genome harbors 5 genes coding for ADHs that could catalyze the conversion of ethanol to acetaldehyde using NAD+ or NADP+ as a cofactor [31, 32].
Ethanol production by the wild-type strain S. ovata DSM-2662 used here was recently reported for the first time during gas fermentation in a gas liquid (GLC) contactor system with a continuous flow of H2 and CO2. High yield of acetate was also obtained with the GLC system. In Blanchet et al.  study, yeast extract was added to the 311 standard cultivation medium, which probably resulted in bacterial cultures with higher cell densities contributing to the high productivity observed. However, utilization of yeast extract in the GLC system makes performance comparison difficult, since no yeast extract was added to other S. ovata-driven bioproduction processes from CO2 including MES [3, 25, 26, 34–36]. More surprisingly, Blanchet et al. indicated that in their study yeast extract was essential for the growth of S. ovata DSM-2662, although autotrophic growth without yeast extract is a well-established defining characteristic of this strain [3, 37].
Involvement of AORs in the conversion of acetate to ethanol in S. ovata
Production of ethanol by acetogens from H2 and CO2 has been predicted to have a positive energy balance, if acetate produced from acetyl-CoA is re-assimilated by an AOR to acetaldehyde that will be in turn reduced to ethanol by an ADH (Fig. 4). There is another well-known pathway for ethanol synthesis from acetyl-CoA usually found in heterotrophic microorganisms, which is mediated by a bifunctional aldehyde/alcohol dehydrogenase. However, this pathway would not be energetically favorable in acetogens growing with H2:CO2 . Thus, for the autotrophic production of ethanol by S. ovata, AOR is likely involved. This is supported by the observation presented in this study that optimal ethanol production is dependent on the concentration of tungstate in the medium, since AORs use tungsten as a cofactor .
Six genes annotated as AOR are found in S. ovata genome: aor1 (SOV_1c05650), aor2 (SOV_1c05680), aor3 (SOV_1c12520), aor4 (SOV_5c02820), mop1 (SOV_1c12600), and mop2 (SOV_1c12660) (Fig. 4) . All six AORs are predicted to be tungsten-containing enzymes. S. ovata also possesses five genes coding for ADH. To further understand the impact of tungstate concentration on the ethanol biosynthesis pathway in S. ovata, RT-qPCR was conducted to measure the transcript abundance of AOR- and ADH-coding genes in the exponential growth phase of S. ovata cultures growing on H2:CO2 (Fig. 5).
The sequence alignment of Aor1 and Aor2 showed that Aor2 (484 AA) is identical to the C-terminal part of Aor1 (from position 96 to 579 out of 579 AA). Attempts to develop a RT-qPCR assay targeting the 5′ gene region unique to aor1 failed. Thus, transcript abundance variation was investigated using a pair of primers targeting both aor1 and aor2 (Additional file 1: Table S1). In the presence of 10× tungstate, transcript abundance of aor1–2 was significantly increased by 30.4 ± 9.8-fold. Moreover, aor4 and mop2 were also upregulated by 14.3 ± 5.6-fold and 3.8 ± 0.4-fold, respectively (Fig. 5a). In contrast, no significant change in the expression of aor3 and mop1 was observed. Transcript abundance of the five genes coding for ADHs also remained the same in the presence of 1× or 10× tungstate (Fig. 5b). Results presented here suggest that tungstate was in limiting concentration in standard 311 medium and optimizing tungstate concentration enabled higher expression of the AORs encoded by aor1, aor2, aor4, and mop2, which subsequently augmented the enzymatic capacity of S. ovata for the conversion of acetate to acetaldehyde possibly leading to higher ethanol production.
Transcript abundance of genes coding for tungsten-containing FDH
Among the metalloenzymes involved in the WL pathway, tungsten is known to be a cofactor for acetogenic FDHs [16, 39, 40]. Hence, RT-qPCR was employed to determine the impact of augmenting tungstate concentration under autotrophic conditions on the transcript abundance of genes fdhA1 (SOV_1c07830) and fdhA2 (SOV_3c08790). fdhA1 and fdhA2 are coding for α-subunits of the two FDHs of S. ovata. Transcript abundance of fdhA2 was increased 3.3 ± 0.2-fold when tungstate concentration was decupled, whereas the expression of fdhA1 remained the same (Fig. 5c). Augmentation of the expression of FdhA2 in S. ovata may cause increase in the carbon flux from CO2 to acetyl-CoA via the WL pathway and thus contributes to the improved growth as well as the higher ethanol production associated with optimal tungstate concentration.
The conversion of longer carbon chain fatty acids to alcohols by S. ovata during gas fermentation
AORs can convert multiple fatty acids other than acetate including propionic and butyric acids to their respective aldehydes, which will be subsequently converted to alcohols . The presence of six AORs in S. ovata suggests that this acetogen has the enzymatic potential for the biosynthesis of longer alcohols than ethanol. To determine if other fatty acids could be converted to aldehydes and then alcohols by S. ovata and also to verify if these reactions are associated with the presence of tungstate like the production of ethanol, 5 mM of propionic acid or 5 mM of butyric acid was added to S. ovata cultures under H2:CO2 growth condition in the presence of 1× or 10× tungstate concentration. Addition of propionate resulted in the generation of 1-propanol, whereas addition of butyrate led to the synthesis of 1-butanol (Table 2). Conversion of propionate to 1-propanol reached a final efficiency of 20.6 ± 4.1 % in a standard tungstate concentration medium after 380 h. When 10× more tungstate was present in the medium, conversion efficiency was increased by 1.6-fold (Table 2). Similarly, a higher conversion of butyric acid to 1-butanol was observed with decupled tungstate and the conversion efficiency was increased by 1.3-fold compared with standard tungstate medium (Table 2). Unpaired t test was used to evaluate the statistical significance of the fold increases in conversion efficiency observed in the presence of 10× tungstate. The p values for both fold changes in propanol and 1-butanol production was below 0.05 confirming statistical significance. These results indicate that S. ovata possesses AORs and ADHs that can convert multiple fatty acids to alcohols in a tungsten-associated manner. It also shows that S. ovata has the metabolic capacity for the reduction of longer fatty acids than acetate into alcohols, which could be harnessed to develop novel bioproduction processes.
Increasing interest for acetogens in the recent years is mainly driven by the development of new technologies aiming to use CO2 waste gases as feedstock for the production of valuable organic carbon compounds [4, 41]. In this study, a simple optimization of tungstate concentration in S. ovata cultivation medium significantly improved the conversion of CO2 to acetate by MES and also promoted the production of ethanol during autotrophic growth on H2:CO2 or by MES. Furthermore, increasing tungstate concentration resulted in higher transcript abundance of genes coding for AORs strongly suggesting their participation in the ethanol biosynthesis pathway of S. ovata. In addition, a gene coding for tungsten-containing FDH was upregulated, indicating that augmenting tungstate concentration in the medium possibly increased the carbon flux in the WL pathway of S. ovata leading to increased growth and improved productivity. Successful conversion of longer carbon chain fatty acids to alcohols by S. ovata during gas fermentation reveals that AORs and ADHs of S. ovata can participate to the biosynthesis of longer alcohols than ethanol, and it also highlights the potential of this species for the bioproduction from CO2 of valuable chemicals other than acetate and ethanol. Further understanding and optimization of the AOR-associated pathways of S. ovata involved in alcohols production from fatty acids could lead to the bioengineering of highly efficient biocatalysts for the production of biofuels via MES or via other types of biosystems.
Bacterial strain, growth conditions, media modifications, and fatty acids conversion
The bacterium S. ovata DSM-2662  was obtained from the Deutsche Sammlung Mikroorganismen und Zellkulturen (DMSZ). S. ovata cultures were routinely grown under a H2:CO2 (80:20) atmosphere (1.7 atm) at 30 °C in stoppered and crimp-sealed tubes. The medium DSMZ 311 used for cultivation was prepared under strict anaerobic condition. Yeast extract, casitone, betaine, resazurin, and sodium sulfide were all omitted from 311 medium. Trace elements investigated in this study are presented in Table 3 with their standard 1× concentrations in 311 medium. Growth was determined by measuring optical density (OD) at 545 nm with an Evolution™ 202 UV–Visible spectrophotometer (Thermo Scientific, Denmark). Conversion of fatty acids to alcohols by S. ovata during gas fermentation was carried out in 311 medium containing 5 mM propionic acid or 5 mM butyric acid and 0.01 µM or 0.1 µM of tungstate. All experiments were conducted at least in triplicate.
Electrosynthesis of acetate and ethanol by MES
MES experiment was operated at 25 °C in a dual-chambered H-type reactor consisting of three-electrode with S. ovata inoculated in the cathodic chamber as previously described [3, 25]. The cathodic chamber and the anodic chamber were filled with a final volume of 300 ml of 311 medium containing 1× or 10× tungstate. The two chambers were separated by a Nafion 115 membrane (Ion Power, Inc., New Castle, DE, USA). Both the anode (36 cm2), and the cathode (36 cm2) were graphite sticks suspended in the culture medium. 100 ml of S. ovata cells pre-grown in 311 medium with 1× or 10× tungstate under a H2:CO2 atmosphere was injected into the cathodic chamber containing 200 ml of 311 medium with corresponding tungstate concentration. The cathode potential was set at −690 mV versus SHE with a potentiostat (ECM8, Gamry Instruments, PA, USA). During MES, both chambers of H-type reactors were continually bubbled with N2:CO2 (80:20). MES experiments were repeated in triplicate. Acetate and ethanol production rates were normalized with respect to the projected surface area of the graphite stick cathode.
Acetate, propionate, and butyrate were measured with an Ultimate 3000 high-pressure liquid chromatography system (Thermo Scientific, Denmark) equipped with an Aminex HPX-87H anion exchange column (Bio-Rad, California) set at a temperature of 30 °C. 5 mM H2SO4 was used as the mobile phase at a flow rate of 0.6 ml/min. Ethanol, 1-propanol, and 1-butanol were quantified with a Trace 1300 gas chromatograph (Thermo Scientific, Denmark) equipped with a flame ionization detector with the temperature set at 300 °C. Samples were injected into an Rtx-Wax column (fused silica, 30 m × 0.25 mm × 0.25 µM). (Restek, PA, USA). The injector port temperature was set at 250 °C. The oven temperature was programmed to 40 °C for 2 min, followed by an increase of 10 °C per minute until reaching 200 °C. All results presented in this study are from at least three independent experiments.
Quantitative reverse transcription PCR (RT-qPCR)
Transcript abundance of AOR-, ADH-, and FDH α-subunit-coding genes was compared by RT-qPCR in S. ovata cultures grown under a H2:CO2 atmosphere in 311 medium containing 1× or 10× tungstate. AOR-coding genes in S. ovata DSM-2662 are aor1 (SOV_1c05650), aor2 (SOV_1c05680), aor3 (SOV_1c12520), aor4 (SOV_5c02820), mop1 (SOV_1c12600) and mop2 (SOV_1c12660). ADH-coding genes are SOV_1c02190, adh (SOV_1c05680), SOV_2c03040, SOV_3c00580 and adhB (SOV_3c00590). FDH α-subunit-coding genes are fdhA1 (SOV_1c07830) and fdhA2 (SOV_3c08790). Expression of these genes were normalized with polC1 (SOV_1c12130), a housekeeping gene constitutively expressed under the tested conditions coding for the DNA polymerase III. Primer 3 software was used to design primers for RT-qPCR (Additional file 1: Table S1) . Total RNA was extracted from triplicate S. ovata cultures in the exponential growth phase after 3 days. Briefly, bacterial cultures were centrifuged and cell pellets were suspended in Trizol®Max Bacterial Enhancement Reagent (Ambion). Extraction of Total RNA was done with Trizol® Reagent (Ambion) according to manufacturer’s instructions. The absence of DNA contamination in total RNA extracts was verif1ied by the absence of PCR amplification with the polIII-F and polIII-R primers. cDNA was generated with Superscript III Reverse Transcriptase (Invitrogen) using random primers. RT-qPCR was carried out with Brilliant III Ultra-Fast SYBR® Green qPCR Master Mix (Agilent Technologies). Each RT-qPCR reaction was carried out at least in triplicate with an Mx3005P qPCR system (Agilent technologies). Relative expression levels of different genes were measured using Pfaffl mathematical model for relative quantification . Fold changes over 2 or under 0.5 were considered significant transcript abundance variations.
aldehyde ferredoxin oxidoreductase
quantitative reverse transcription PCR
Ragsdale SW, Pierce E. Acetogenesis and the Wood–Ljungdahl pathway of CO2 fixation. Biochim Biophys Acta. 2008;1784:1873–98.
Lovley DR, Nevin KP. Electrobiocommodities: powering microbial production of fuels and commodity chemicals from carbon dioxide with electricity. Curr Opin Biotechnol. 2013;24:385–90.
Nevin KP, Woodard TL, Franks AE, Summers ZM, Lovley DR. Microbial electrosynthesis: feeding microbes electricity to convert carbon dioxide and water to multicarbon extracellular organic compounds. MBio. 2010;1:e00103–10.
Tremblay P-L, Zhang T. Electrifying microbes for the production of chemicals. Front Microbiol. 2015;6:201.
Daniell J, Köpke M, Simpson SD. Commercial biomass syngas fermentation. Energies. 2012;5:5372–417.
Atomi H. Microbial enzymes involved in carbon dioxide fixation. J Biosci Bioeng. 2002;94:497–505.
Drake HL, Gößner AS, Daniel SL. Old acetogens, new light. Ann NY Acad Sci. 2008;1125:100–28.
Saxena J, Tanner RS. Optimization of a corn steep medium for production of ethanol from synthesis gas fermentation by Clostridium ragsdalei. World J Microbiol Biotechnol. 2012;28:1553–61.
Gao J, Atiyeh HK, Phillips JR, Wilkins MR, Huhnke RL. Development of low cost medium for ethanol production from syngas by Clostridium ragsdalei. Bioresour Technol. 2013;147:508–15.
Phillips JR, Atiyeh HK, Tanner RS, Torres JR, Saxena J, Wilkins MR, et al. Butanol and hexanol production in Clostridium carboxidivorans syngas fermentation: medium development and culture techniques. Bioresour Technol. 2015;190:114–21.
Saxena J, Tanner RS. Effect of trace metals on ethanol production from synthesis gas by the ethanologenic acetogen Clostridium ragsdalei. J Ind Microbiol Biotechnol. 2011;38:513–21.
Bender G, Pierce E, Hill JA, Darty JE, Ragsdale SW. Metal centers in the anaerobic microbial metabolism of CO and CO2. Met Integr Biometal Sci. 2011;3:797–815.
Cammack R. Bioinorganic chemistry: hydrogenase sophistication. Nature. 1999;397:214–5.
Andreesen JR, Makdessi K. Tungsten, the surprisingly positively acting heavy metal element for prokaryotes. Ann NY Acad Sci. 2008;1125:215–29.
Andreesen JR, Ljungdahl LG. Formate dehydrogenase of Clostridium thermoaceticum: incorporation of selenium-75, and the effects of selenite, molybdate, and tungstate on the enzyme. J Bacteriol. 1973;116:867–73.
Yamamoto I, Saiki T, Liu SM, Ljungdahl LG. Purification and properties of NADP-dependent formate dehydrogenase from Clostridium thermoaceticum, a tungsten–selenium–iron protein. J Biol Chem. 1983;258:1826–32.
Zhu X, Tan X. Metalloproteins/metalloenzymes for the synthesis of acetyl-CoA in the Wood–Ljungdahl pathway. Sci China, Ser B: Chem. 2009;52:2071–82.
Drennan CL, Doukov TI, Ragsdale SW. The metalloclusters of carbon monoxide dehydrogenase/acetyl-CoA synthase: a story in pictures. J Biol Inorg Chem. 2004;9:511–5.
Scopes RK. An iron-activated alcohol dehydrogenase. FEBS Lett. 1983;156:303–6.
Korkhin Y, Kalb AJ, Peretz M, Bogin O, Burstein Y, Frolow F. NADP-dependent bacterial alcohol dehydrogenases: crystal structure, cofactor-binding and cofactor specificity of the ADHs of Clostridium beijerinckii and Thermoanaerobacter brockii. J Mol Biol. 1998;278:967–81.
Bertsch J, Müller V. Bioenergetic constraints for conversion of syngas to biofuels in acetogenic bacteria. Biotechnol Biofuels. 2015;8:210.
Kletzin A, Adams MW. Tungsten in biological systems. FEMS Microbiol Rev. 1996;18:5–63.
Lvov NP, Nosikov AN, Antipov AN. Tungsten-containing enzymes. Biochemistry. 2002;67:196–200.
Sevcenco A-M, Bevers LE, Pinkse MWH, Krijger GC, Wolterbeek HT, Verhaert PDEM, et al. Molybdenum incorporation in tungsten aldehyde oxidoreductase enzymes from Pyrococcus furiosus. J Bacteriol. 2010;192:4143–52.
Tremblay P-L, Höglund D, Koza A, Bonde I, Zhang T. Adaptation of the autotrophic acetogen Sporomusa ovata to methanol accelerates the conversion of CO2 to organic products. Sci. Rep. 2015;5:16168.
Chen L, Tremblay P-L, Mohanty S, Xu K, Zhang T. Electrosynthesis of acetate from CO2 by a highly structured biofilm assembled with reduced graphene oxide–tetraethylene pentamine. J Mater Chem A. 2016;4:8395–401.
Buschhorn H, Dürre P, Gottschalk G. Production and utilization of ethanol by the homoacetogen Acetobacterium woodii. Appl Environ Microbiol. 1989;55:1835–40.
Monot F, Martin JR, Petitdemange H, Gay R. Acetone and butanol production by Clostridium acetobutylicum in a synthetic medium. Appl Environ Microbiol. 1982;44:1318–24.
Amador-Noguez D, Brasg IA, Feng X-J, Roquet N, Rabinowitz JD. Metabolome remodeling during the acidogenic-solventogenic transition in Clostridium acetobutylicum. Appl Environ Microbiol. 2011;77:7984–97.
Isom CE, Nanny MA, Tanner RS. Improved conversion efficiencies for n-fatty acid reduction to primary alcohols by the solventogenic acetogen “Clostridium ragsdalei”. J Ind Microbiol Biotechnol. 2015;42:29–38.
Möller B, Oßmer R, Howard BH, Gottschalk G, Hippe H. Sporomusa, a new genus of gram-negative anaerobic bacteria including Sporomusa sphaeroides spec. nov. and Sporomusa ovata spec. nov. Arch Microbiol. 1984;139:388–96.
Poehlein A, Gottschalk G, Daniel R. First insights into the genome of the gram-negative, endospore-forming organism Sporomusa ovata strain H1 DSM 2662. Genome Announc. 2013;1:e00734.
Blanchet E, Duquenne F, Rafrafi Y, Etcheverry L, Erable B, Bergel A. Importance of the hydrogen route in up-scaling electrosynthesis for microbial CO2 reduction. Energy Environ Sci. 2015;8:3731–44.
Nie H, Zhang T, Cui M, Lu H, Lovley DR, Russell TP. Improved cathode for high efficient microbial-catalyzed reduction in microbial electrosynthesis cells. Phys Chem Chem Phys. 2013;15:14290–4.
Giddings CGS, Nevin KP, Woodward T, Lovley DR, Butler CS. Simplifying microbial electrosynthesis reactor design. Front Microbiol. 2015;6:468.
Zhang T, Nie H, Bain TS, Lu H, Cui M, Snoeyenbos-West OL, et al. Improved cathode materials for microbial electrosynthesis. Energy Environ Sci. 2013;6:217–24.
Vos P, Garrity G, Jones D, Krieg NR, Ludwig W, Rainey FA, et al. Bergey’s Manual of Systematic Bacteriology: Volume 3: the firmicutes. Berlin: Springer Science & Business Media; 2011.
Chan MK, Mukund S, Kletzin A, Adams MW, Rees DC. Structure of a hyperthermophilic tungstopterin enzyme, aldehyde ferredoxin oxidoreductase. Science. 1995;267:1463–9.
Ljungdahl LG, Andreesen JR. Formate dehydrogenase, a selenium–tungsten enzyme from Clostridium thermoaceticum. Methods Enzymol. 1978;53:360–72.
Alissandratos A, Kim H-K, Matthews H, Hennessy JE, Philbrook A, Easton CJ. Clostridium carboxidivorans strain P7T recombinant formate dehydrogenase catalyzes reduction of CO2 to formate. Appl Environ Microbiol. 2013;79:741–4.
Daniell J, Nagaraju S, Burton F, Köpke M, Simpson SD. Low-carbon fuel and chemical production by anaerobic gas fermentation. Adv. Biochem Eng Biotechnol. 2016. doi: 10.1007/10_2015_5005
Rozen S, Skaletsky H. Primer3 on the WWW for general users and for biologist programmers. Methods Mol Biol. 2000;132:365–86.
Pfaffl MW. A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Res. 2001;29:e45.
FA, PLT, and TZ conceived the study. FA, DML, and TZ performed all the experimental work. FA, PLT, and TZ interpreted the data and wrote the manuscript. All the authors read and approved the final manuscript.
The authors declare that they have no competing interests.
This work was funded by the Novo Nordisk Foundation.