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Applied and Environmental Microbiology, March 2007, p. 1420-1424, Vol. 73, No. 5
0099-2240/07/$08.00+0     doi:10.1128/AEM.02508-06
Copyright © 2007, American Society for Microbiology. All Rights Reserved.

Growth Yields in Bacterial Denitrification and Nitrate Ammonification

Tobin O. Strohm,¹ Ben Griffin,^1, Walter G. Zumft,² and Bernhard Schink^1*

Fachbereich Biologie, Universität Konstanz, D-78457 Konstanz, Germany,¹ Lehrstuhl für Mikrobiologie, Universität Karlsruhe, D-76128 Karlsruhe, Germany²

Received 27 October 2006/ Accepted 22 December 2006

Top Abstract Introduction Materials and Methods Results Discussion References

 
Denitrification and nitrate ammonification are considered the highest-energy-yielding respiration systems in anoxic environments after oxygen has been consumed. The corresponding free energy changes are 7 and 35% lower than that of aerobic respiration, respectively. Growth yield determinations with pure cultures of Paracoccus denitrificans and Pseudomonas stutzeri revealed that far less energy is converted via ATP into cell mass than expected from the above calculations. Denitrification with formate or hydrogen as electron donor yielded about 2.4 to 3.0 g dry matter per mol formate or hydrogen and 15 to 18 g dry matter per mol acetate. Similar yields with acetate were obtained with Pseudomonas stutzeri. Wolinella succinogenes and Sulfurospirillum deleyianum, which reduce nitrate to ammonia, both exhibited similar yield values with formate or H₂ plus nitrate. The results indicate that ATP synthesis in denitrification is far lower than expected from the free energy changes and even lower than in nitrate ammonification. The results are discussed against the background of our present understanding of electron flow in denitrification and with respect to the importance of denitrification and nitrate ammonification in the environment.

Top Abstract Introduction Materials and Methods Results Discussion References

 
Oxidation of biomass proceeds preferentially with oxygen as electron acceptor, and only after its consumption in deeper sediment layers are alternative electron acceptors such as nitrate, manganese(IV), ferric iron, sulfate, or CO₂ reduced (15, 30). After oxygen reduction, reduction of nitrate to N₂ (denitrification) or to ammonia (nitrate ammonification) is the highest-energy-yielding process as shown by the following equations calculated with glucose as a representative of biomass (calculated based on the tables in reference 25):

(1)

(2)

(3)

Even if we assume substrate and product concentrations more appropriate to natural conditions, i.e., 1 µM glucose and 10 µM nitrate and ammonium, the free energies of reactions 1 and 3 change by +34 kJ and that of equation 2 changes by +171 kJ, which still leaves a substantially higher amount of free energy with the denitrification process. From this comparison, one would expect that ATP synthesis as measured via growth yields in denitrification should come close to that of aerobic respiration, and yields in nitrate ammonification should be substantially lower. Thus, denitrification is expected to be the preferred process over nitrate ammonification, especially if the overall energy yield of a metabolic process is low. Contrary to this assumption, nitrate ammonification was reported to be the preferred process in anoxic environments in which the nitrate supply is limiting (26, 27). Moreover, nearly all recently described lithotrophic bacteria oxidizing sulfide with nitrate as electron acceptor at neutral pH, e.g., Thioploca sp. or Thiomargarita sp., convert nitrate to ammonia (12, 16, 17), although denitrification should provide them with more energy.

The energetics of nitrate reduction and the mechanisms of energy conservation in this process have been discussed in the past in great detail (22, 24). Growth yields of nitrate-reducing bacteria have been determined repeatedly but always with complex substrates such as sugars, succinate, or glutamate (9, 10, 23), and not in all cases were the experimental conditions documented clearly enough to identify the limiting substrate and to verify whether nitrate was reduced completely. Later the structural organization of the electron transfer components within and outside the cytoplasmic membrane was resolved (6, 32), but the implications of these findings for the overall energy balance of denitrification remained unclear. We therefore undertook a comparative evaluation of growth yields with well-described denitrifying and ammonifying bacteria in mineral media with simple substrates such as acetate, H₂, and formate under directly comparable conditions in order to obtain reliable data for a comparison of growth yields of these two important anaerobic respiratory processes.

Top Abstract Introduction Materials and Methods Results Discussion References

 
Organisms and cultivation.
Paracoccus denitrificans (DSM 65^T), Pseudomonas stutzeri (DSM 5190^T), and Sulfurospirillum deleyianum (DSM 6946^T) were obtained from Deutsche Sammlung von Mikroorganismen und Zellkulturen GmbH, Braunschweig, Germany. Wolinella succinogenes (DSM 1740^T) was a kind gift of the lab of Achim Kröger, Frankfurt, Germany.

P. denitrificans and P. stutzeri were grown in oxygen-free nonreduced bicarbonate-buffered mineral salts medium (13). S. deleyianum and W. succinogenes were grown in bicarbonate-buffered sulfide-reduced mineral salts medium as described earlier (14, 29). Growth experiments were carried out at least in duplicate (most in four to six independent assays) in 22-ml Hungate tubes sealed with butyl rubber stoppers and filled with 10 ml culture medium under a headspace of N₂/CO₂ (80%/20%) or in tubes completely filled with medium and closed with latex-sealed screw caps. With gaseous substrates, tubes were incubated lying on a shaker at about 60 rpm. Growth was followed via turbidity measurement with a Spectronics 70 spectrophotometer at a 546-nm wavelength (Bausch & Lomb, Rochester, NY). Turbidity was followed at intervals of 4 to 12 h for up to 10 days. Growth yield determinations were calibrated by gravimetric determination of dry cell mass grown in 1-liter cultures.

Biochemical analysis of acetate activation.
Cells of P. denitrificans and P. stutzeri were harvested in 1-liter cultures in the late exponential growth phase and washed with oxygen-free 100 mM Tris-HCl buffer, pH 7.8, containing 5 mM MgCl₂ and 2 mM dithiothreitol. Cells were broken by repeated French press treatment anoxically under N₂, and cell debris was removed by centrifugation at 10,000 x g for 10 min. The membrane fraction was removed by centrifugation at 100,000 x g for 45 min. The supernatant contained the cytoplasmic and the periplasmic fraction. Synthesis of acetyl coenzyme A (acetyl-CoA) from acetate, ATP, and coenzyme A was followed in a coupled photometric assay including myokinase, phosphoenolpyruvate, and NADH (31). The stoichiometry of NADH oxidation over acetate consumption was assayed with limiting amounts (0.1 mM) of acetate.

Chemicals.
Chemicals used were of analytical grade and were obtained from Fluka (Buchs, Switzerland), Riedel-de Haën (Seelze, Germany), and Merck (Darmstadt, Germany). Biochemicals were purchased from Sigma (München, Germany).

Top Abstract Introduction Materials and Methods Results Discussion References

 
Determination of conversion factors.
Conversion factors for calculation of cell yields from optical density (OD) values were determined in 1-liter cultures. The conversion factors obtained were very similar for all bacteria used. An OD value at 546 nm (OD₅₄₆) of 0.1 measured against a medium blank corresponded to 24.0 mg (dry weight) of cells per liter with P. denitrificans, 23.5 mg (dry weight) of cells per liter with P. stutzeri, 24.8 mg (dry weight) of cells per liter with W. succinogenes, and 24.3 mg (dry weight) of cells per liter with S. deleyianum. These calibration factors were identical also after growth with different substrates because the cell shape of these bacteria is very constant. These values were used for calculations of cell yields in the subsequent experiments.

Growth experiments.
P. denitrificans grew with acetate plus nitrate with doubling times of 4 to 6 h. With formate, doubling times were about 10 h, and with hydrogen they were about 20 h. Growth yields were determined with P. denitrificans in static cultures with either acetate, formate, or hydrogen as electron donor and either nitrate, nitrite, or N₂O as electron acceptor. As reported in Table 1, growth yields with acetate plus nitrate were about 15 to 18 g per mol acetate or 9.4 to 11.3 g per mol nitrate, no matter whether acetate or nitrate was the limiting substrate, indicating that nitrate was completely reduced to N₂. With formate or hydrogen as electron donor, yields were considerably smaller, with 2.4 to 3.0 g per mol formate or H₂ and 6.0 to 7.6 g per mol nitrate. With nitrite as electron acceptor, the yields were substantially higher, 18 to 25 g per mol acetate, and were lower with N₂O. Similar yield determinations were carried out with Pseudomonas stutzeri, another well-studied nitrate reducer which oxidizes only organic compounds such as acetate. The growth yields obtained (Table 2) were similar to those found with P. denitrificans on acetate, indicating that these results may be taken as representative of denitrifying bacteria in general.

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TABLE 1. Growth experiments with P. denitrificansa

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TABLE 2. Growth experiments with P. stutzeria

Growth yields were also determined with the nitrate-ammonifying bacteria W. succinogenes and S. deleyianum. As shown in Table 3, nitrate reduction with formate or H₂ as electron donor by W. succinogenes yielded about 4 g cell mass per mol formate and 1.7 g per mol H₂ with nitrate as electron acceptor; with fumarate or nitrite as electron acceptor, the obtained yields were slightly higher or lower, respectively. Since W. succinogenes has to be grown in a sulfide-reduced medium, care has to be taken with growth studies in the presence of excess electron acceptor: Turbidity develops quickly after transfer, but this turbidity is caused not by cell growth but by partial oxidation of sulfide to elemental sulfur. W. succinogenes also turned out to be quite sensitive to enhanced nitrite additions: no growth was observed at nitrite concentrations higher than 3 mM nitrite, and growth was inhibited by nitrite accumulating in cultures with excess nitrate. Growth yields obtained with S. deleyianum with formate as electron donor and nitrate as electron acceptor were nearly identical to those obtained with W. succinogenes (results not shown).

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TABLE 3. Growth experiments with W. succinogenesa

Acetate activation by P. denitrificans and P. stutzeri.
The enzyme system responsible for activation of acetate to acetyl-CoA was identified in P. denitrificans cytoplasm. The coupled assay system (31) revealed that 0.206 mM NADH was oxidized per 0.1 mM acetate supplied, indicating that two ATP equivalents were consumed in acetate synthesis, as typical of an acetate-CoA ligase enzyme (acetyl-CoA synthetase, EC 6.2.1.1) forming AMP and pyrophosphate (with subsequent hydrolysis) from ATP in acetyl-CoA synthesis. Similar results were obtained with extracts of P. stutzeri.

Top Abstract Introduction Materials and Methods Results Discussion References

 
Our results clearly document that the energy yields of nitrate reduction are far lower than one would expect from the free energy changes of the overall redox reactions (see above). Although similar studies have been carried out in the past, yield determinations in denitrification and nitrate ammonification under directly comparable conditions in defined mineral media have not been carried out so far. Detailed studies of the bioenergetics of Wolinella succinogenes have been performed in the past, and our yield values confirm those obtained in those studies (2, 20). These authors documented in detail that formate-dependent growth of W. succinogenes with nitrate as electron acceptor yields less cell mass than formate oxidation with fumarate does, although the free energy change of the latter reaction is substantially lower than that of nitrate ammonification. The corresponding ATP yields were calculated to be 0.43 ATP per mol formate with nitrate or 0.72 ATP per mol formate with fumarate as electron acceptor (2, 20). Hydrogen-dependent nitrate ammonification by the sulfate reducer Desulfovibrio desulfuricans yields 5.2 g cell mass per mol hydrogen in static culture conditions, which is equivalent to about 0.5 ATP per mol (19).

Growth yields in denitrification have been determined in the past mainly with sugars and other more complex substrates (9, 10, 22, 23). Phosphorylation efficiencies measured with membrane vesicles of P. denitrificans were found to be 0.9 P per NADH (8, 11).

The molecular organization of the nitrate-reducing enzyme apparatus of denitrifying bacteria has been worked out in regard to its biochemistry and its molecular organization (4, 6, 32); a general concept of the electron transport system is depicted in Fig. 1, which is based on similar schemes by Ferguson (6) and Zumft (32). For comparison, one should take into account that in the aerobic respiratory chain of mitochondria and many aerobic bacteria, a total of 10 H⁺ are transported across the membrane per NADH electron pair, 4 H⁺ in the NADH dehydrogenase reaction, 2 H⁺ in the quinone cycle, 2 H⁺ in the cytochrome bc₁ complex, and 2 H⁺ in the cytochrome oxidase reaction (7, 28). Reduction of nitrate to N₂, on the other hand, proceeds through four different reductase enzymes: nitrate reductase, NADH dehydrogenase, and NO reductase are integral membrane proteins whereas nitrite reductase and N₂O reductase are located in the periplasm. NADH dehydrogenase and the cytochrome bc₁ complex are considered to be active proton pumps, and the ubiquinone cycles connecting either to nitrate reductase or to the cytochrome bc₁ complex are supposed to translocate protons as well. The other reductases do not contribute to proton translocation; rather, they consume protons in the periplasmic space. Nonetheless, this proton consumption does not influence the ATP yield significantly because the pH in the periplasm is maintained by the medium buffer.

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FIG. 1. Organization of respiratory elements involved in denitrification by Paracoccus denitrificans and the impact of proton translocation across the membrane. The figure is redrawn from similar schemes by Ferguson (6) and Zumft (32). Abbreviations: AP, antiporter; NAR, nitrate reductase b; UQ, ubiquinone; DH, NADH dehydrogenase; Cyt bc1, cytochrome bc1 complex; NOR, NO reductase; NO2– RED, nitrite reductase; N2O RED, N2O reductase; Cyt c550, cytochrome c550.

Reduction of two molecules of nitrate to N₂ with five NADH molecules as electron donor translocates a total of 36 protons across the membrane. If we assume that four protons are required for synthesis of one ATP molecule (3, 5, 18), nine ATP molecules can be synthesized with the electrons of five NADH molecules, i.e., 1.8 ATP is synthesized per NADH, which would be twice as much as the value (0.9) obtained by the study in reference 8.

Hydrogen and formate are oxidized on the outer face of the cytoplasmic membrane and donate electrons to quinones, leaving two protons per two electrons in the periplasm (20); the proton balances and ATP yields with these substrates are therefore lower than those obtained with NADH as electron donor (26 H⁺ per 10 e^–, or 1.3 ATP per two electrons). From the average molar growth yield with formate or H₂, Y_ATP can be estimated to be about 2.3 g per mol ATP. This value is typical of a bacterium which has to synthesize its cell material autotrophically from CO₂ or formate via the Calvin cycle (21).

Acetate oxidation in the citric acid cycle yields three electron pairs at the NADH level and one at the ubiquinone level. The total proton balance for ubiquinol-dependent nitrate reduction is 16 protons translocated per five ubiquinol molecules oxidized. This leads to a total of 24.8 protons per acetate oxidized, corresponding to 6.2 ATP formed by electron transport phosphorylation. Two ATP equivalents are consumed in acetate activation as confirmed in our study, and one ATP molecule is gained in the citric acid cycle in the succinate thiokinase reaction, leaving a total of 5.2 ATP per mol acetate. Our growth yields agree with this assumption, giving a Y_ATP value of 3.3 g per mol ATP, which is low for heterotrophic growth in a mineral medium with a simple substrate like acetate (21).

Growth yields with nitrite or N₂O as electron acceptor were in the same range as those with nitrate. Indeed, reduction of nitrite, NO, and N₂O translocates similar amounts of protons per NADH or ubiquinol oxidized as does nitrate reduction to N₂ (Fig. 1). These results confirm basically earlier findings (9, 10) that the three main steps in denitrification release about equal amounts of energy.

A comparison of growth yields between P. denitrificans and W. succinogenes makes it obvious that denitrification yields slightly lower rather than higher cell amounts than nitrate ammonification does. This becomes even more pronounced if the yields are calculated per mol electron acceptor: since reduction of nitrate to ammonia consumes eight electrons rather than five in denitrification, the energy yield per nitrate reduced is higher for nitrate ammonification than for denitrification:

(4)

(5)

In our experiments it appears that about twice as much cell mass can be synthesized per mol nitrate by nitrate ammonification as by denitrification (15.6 versus 7.6 g per nitrate reduced with formate as electron donor; Tables 1 and 3). Thus, it is not surprising that nitrate ammonification is the preferred nitrate respiration process under conditions of nitrate limitation (26) and that especially lithoautotrophic sulfide oxidation by, e.g., Thioploca sp. or Thiomargarita sp. prefers nitrate ammonification over denitrification (12, 16, 17).

The observed inefficient energy conservation in the reduction of nitrite to nitrogen gas may also explain why no bacterium has been described so far which grows by dismutation of nitrite to nitrate plus N₂ although this reaction yields substantial amounts of energy:

(6)

The analogous dismutation of sulfite to sulfate plus sulfide, yielding a similar amount of energy (G°' = –59 kJ per mol sulfite), was described many years ago as a novel type of "inorganic fermentation" (1). This appears not to work out with nitrite dismutation to N₂ plus nitrate, obviously because the reduction of the most positive electron acceptor systems (reduction of NO and N₂O, at E°' = +1,180 and +1,350 mV, respectively) proceeds in the periplasm, without concomitant energy conservation.

 
We are grateful to Martina Reiss and Christof Reiner, who contributed some of the growth experiments as course students, and to Elisabeth Kayser for technical help. We also appreciate valuable discussions with B. B. Jørgensen and A. Stouthamer.

This study was supported by research funds of the University of Konstanz.

 
* Corresponding author. Mailing address: Fachbereich Biologie, Universität Konstanz, D-78457 Konstanz, Germany. Phone: (49) 7531 882140. Fax: (49) 7531 884047. E-mail: Bernhard.Schink{at}uni-konstanz.de.

Published ahead of print on 5 January 2007.

Present address: Department of Microbiology, University of Illinois Urbana-Champaign, Urbana, IL 61801.

Top Abstract Introduction Materials and Methods Results Discussion References

 

1
1. Bak, F., and H. Cypionka. 1987. A novel type of energy metabolism involving fermentation of inorganic sulphur compounds. Nature 326:891-892.[CrossRef]
2
2. Bokranz, M., J. Katz, I. Schröder, A. M. Roberton, and A. Kröger. 1983. Energy metabolism and biosynthesis of Vibrio succinogenes growing with nitrate or nitrite as terminal electron acceptor. Arch. Microbiol. 135:36-41.[CrossRef]
3
3. Dimroth, P. 2000. Operation of the F₀ motor of the ATP synthase. Biochim. Biophys. Acta 1458:374-386.[Medline]
4
4. Einsle, O., and P. M. Kroneck. 2004. Structural basis of denitrification. Biol. Chem. 385:875-883.[CrossRef][Medline]
5
5. Engelbrecht, S., and W. Junge. 1997. ATP synthase: a tentative structural model. FEBS Lett. 414:485-491.[CrossRef][Medline]
6
6. Ferguson, S. J. 1994. Denitrification and its control. Antonie Leeuwenhoek 66:89-110.[CrossRef][Medline]
7
7. Heldt, H. W. 2003. Pflanzenbiochemie. Spektrum Akademischer Verlag, Heidelberg, Germany.
8
8. John, P., and F. R. Whatley. 1970. Oxidative phosphorylation coupled to oxygen uptake and nitrate reduction in Micrococcus denitrificans. Biochim. Biophys. Acta 216:342-352.[Medline]
9
9. Koike, I., and A. Hattori. 1975. Growth yield of a denitrifying bacterium, Pseudomonas denitrificans, under aerobic and denitrifying conditions. J. Gen. Microbiol. 88:1-10.[Abstract/Free Full Text]
10
10. Koike, I., and A. Hattori. 1975. Energy yield of denitrification: an estimate from growth yield in continuous cultures of Pseudomonas denitrificans under nitrate-, nitrite- and oxide-limited conditions. J. Gen. Microbiol. 88:11-19.[Abstract/Free Full Text]
11
11. Naik, M. S., and D. J. D. Nicholas. 1966. Phosphorylation associated with nitrate and nitrite reduction in Micrococcus denitrificans and Pseudomonas denitrificans. Biochim. Biophys. Acta 113:490-497.[Medline]
12
12. Otte, S., J. G. Kuenen, L. P. Nielsen, H. W. Paerl, J. Zopfi, H. N. Schulz, A. Teske, B. Strotmann, V. A. Gallardo, and B. B. Jørgensen. 1999. Nitrogen, carbon, and sulfur metabolism in natural Thioploca samples. Appl. Environ. Microbiol. 65:3148-3157.[Abstract/Free Full Text]
13
13. Platen, H., and B. Schink. 1989. Anaerobic degradation of acetone and higher ketones via carboxylation by newly isolated denitrifying bacteria. J. Gen. Microbiol. 135:883-891.[Abstract/Free Full Text]
14
14. Schink, B. 1984. Fermentation of 2.3-butanediol by Pelobacter carbinolicus sp. nov. and Pelobacter propionicus sp. nov., and evidence for propionate formation from C₂ compounds. Arch. Microbiol. 137:33-41.[CrossRef]
15
15. Schink, B. 1989. Mikrobielle Lebensgemeinschaften in Gewässersedimenten. Naturwissenschaften 76:364-372.[CrossRef]
16
16. Schulz, H. N., T. Brinkhoff, T. G. Ferdelman, M. H. Marine, A. Teske, and B. B. Jørgensen. 1999. Dense populations of a giant sulfur bacterium in Namibian shelf sediments. Science 284:493-495.[Abstract/Free Full Text]
17
17. Schulz, H. N., and B. B. Jørgensen. 2001. Big bacteria. Annu. Rev. Microbiol. 55:105-137.[CrossRef][Medline]
18
18. Seelert, H., A. Poetsch, N. A. Dencher, A. Engel, H. Stahlberg, and D. J. Müller. 2000. Proton-powered turbine of a plant motor. Nature 405:418-419.[CrossRef][Medline]
19
19. Seitz, H.-J., and H. Cypionka. 1986. Chemolithotrophic growth of Desulfovibrio desulfuricans with hydrogen coupled to ammonification of nitrate and nitrite. Arch. Microbiol. 146:63-67.[CrossRef]
20
20. Simon, J. 2002. Enzymology and bioenergetics of respiratory nitrite ammonification. FEMS Microbiol. Rev. 26:285-309.[CrossRef][Medline]
21
21. Stouthamer, A. H. 1979. The search for correlation between theoretical and experimental growth yields. Int. Rev. Biochem. Microb. Biochem. 21:1-47.
22
22. Stouthamer, A. H. 1988. Dissimilatory reduction of oxidized nitrogen compounds, p. 245-303. In A. J. B. Zehnder (ed.), Biology of anaerobic microorganisms. John Wiley and Sons, New York, NY.
23
23. Stouthamer, A. H. 1988. Bioenergetics and yields with electron acceptors other than oxygen, p. 345-437. In L. E. Erickson and D. Y.-C. Fung (ed.), Handbook on anaerobic fermentations. Marcel Dekker Inc., New York, NY.
24
24. Stouthamer, A. H., A. P. de Boer, J. van der Oost, and R. J. van Spanning. 1997. Emerging principles of inorganic nitrogen metabolism in Paracoccus denitrificans and related bacteria. Antonie Leeuwenhoek 71:33-41.[CrossRef][Medline]
25
25. Thauer, R. K., K. Jungermann, and K. Decker. 1977. Energy conservation in chemotrophic anaerobic bacteria. Bacteriol. Rev. 41:100-180.[Free Full Text]
26
26. Tiedje, J. M. 1988. Ecology of denitrification and dissimilatory nitrate reduction to ammonium, p. 179-244. In A. J. B. Zehnder (ed.), Biology of anaerobic microorganisms. John Wiley and Sons, New York, NY.
27
27. Tiedje, J. M., A. J. Sexstone, D. D. Myrold, and J. A. Robinson. 1982. Denitrification: ecological niches, competition and survival. Antonie Leeuwenhoek 48:569-583.[CrossRef][Medline]
28
28. Tran, Q. H., and G. Unden. 1998. Changes in the proton potential and the cellular energetics of Escherichia coli during growth by aerobic and anaerobic respiration or by fermentation. Eur. J. Biochem. 251:538-543.[Medline]
29
29. Widdel, F., and N. Pfennig. 1981. Studies on dissimilatory sulfate-reducing bacteria that decompose fatty acids. I. Isolation of new sulfate-reducing bacteria enriched with acetate from saline environments. Description of Desulfobacter postgatei gen. nov., sp. nov. Arch. Microbiol. 129:395-400.[CrossRef][Medline]
30
30. Zehnder, A. J. B., and W. Stumm. 1988. Geochemistry and biogeochemistry of anaerobic habitats, p. 1-38. In A. J. B. Zehnder (ed.), Biology of anaerobic microorganisms. John Wiley and Sons, New York, NY.
31
31. Ziegler, K., R. Buder, J. Winter, and G. Fuchs. 1989. Activation of aromatic acids and aerobic 2-aminobenzoate metabolism in a denitrifying Pseudomonas strain. Arch. Microbiol. 151:171-176.[CrossRef]
32
32. Zumft, W. G. 1997. Cell biology and molecular basis of denitrification. Microbiol. Mol. Biol. Rev. 61:533-616.[Abstract]

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Applied and Environmental Microbiology, March 2007, p. 1420-1424, Vol. 73, No. 5
0099-2240/07/$08.00+0     doi:10.1128/AEM.02508-06
Copyright © 2007, American Society for Microbiology. All Rights Reserved.

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