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10 July 2018

Characterization of the First “Candidatus Nitrotoga” Isolate Reveals Metabolic Versatility and Separate Evolution of Widespread Nitrite-Oxidizing Bacteria


Nitrification is a key process of the biogeochemical nitrogen cycle and of biological wastewater treatment. The second step, nitrite oxidation to nitrate, is catalyzed by phylogenetically diverse, chemolithoautotrophic nitrite-oxidizing bacteria (NOB). Uncultured NOB from the genus “Candidatus Nitrotoga” are widespread in natural and engineered ecosystems. Knowledge about their biology is sparse, because no genomic information and no pure “Ca. Nitrotoga” culture was available. Here we obtained the first “Ca. Nitrotoga” isolate from activated sludge. This organism, “Candidatus Nitrotoga fabula,” prefers higher temperatures (>20°C; optimum, 24 to 28°C) than previous “Ca. Nitrotoga” enrichments, which were described as cold-adapted NOB. “Ca. Nitrotoga fabula” also showed an unusually high tolerance to nitrite (activity at 30 mM NO2) and nitrate (up to 25 mM NO3). Nitrite oxidation followed Michaelis-Menten kinetics, with an apparent Km (Km(app)) of ~89 µM nitrite and a Vmax of ~28 µmol of nitrite per mg of protein per h. Key metabolic pathways of “Ca. Nitrotoga fabula” were reconstructed from the closed genome. “Ca. Nitrotoga fabula” possesses a new type of periplasmic nitrite oxidoreductase belonging to a lineage of mostly uncharacterized proteins. This novel enzyme indicates (i) separate evolution of nitrite oxidation in “Ca. Nitrotoga” and other NOB, (ii) the possible existence of phylogenetically diverse, unrecognized NOB, and (iii) together with new metagenomic data, the potential existence of nitrite-oxidizing archaea. For carbon fixation, “Ca. Nitrotoga fabula” uses the Calvin-Benson-Bassham cycle. It also carries genes encoding complete pathways for hydrogen and sulfite oxidation, suggesting that alternative energy metabolisms enable “Ca. Nitrotoga fabula” to survive nitrite depletion and colonize new niches.
IMPORTANCE Nitrite-oxidizing bacteria (NOB) are major players in the biogeochemical nitrogen cycle and critical for wastewater treatment. However, most NOB remain uncultured, and their biology is poorly understood. Here, we obtained the first isolate from the environmentally widespread NOB genus “Candidatus Nitrotoga” and performed a detailed physiological and genomic characterization of this organism (“Candidatus Nitrotoga fabula”). Differences between key phenotypic properties of “Ca. Nitrotoga fabula” and those of previously enriched “Ca. Nitrotoga” members reveal an unexpectedly broad range of physiological adaptations in this genus. Moreover, genes encoding components of energy metabolisms outside nitrification suggest that “Ca. Nitrotoga” are ecologically more flexible than previously anticipated. The identification of a novel nitrite-oxidizing enzyme in “Ca. Nitrotoga fabula” expands our picture of the evolutionary history of nitrification and might lead to discoveries of novel nitrite oxidizers. Altogether, this study provides urgently needed insights into the biology of understudied but environmentally and biotechnologically important microorganisms.


Nitrification, the microbially catalyzed oxidation of ammonia via nitrite to nitrate, is a key process of the natural biogeochemical nitrogen cycle. Nitrification also is critical for the removal of excess nitrogen from sewage in wastewater treatment plants (WWTPs), whereas in agriculture, it contributes to the loss of nitrogen from fertilized soils (1). The first step of nitrification—ammonia oxidation to nitrite—is carried out by chemolithoautotrophic ammonia-oxidizing bacteria and archaea, whereas the second step—nitrite oxidation to nitrate—is catalyzed by chemolithoautotrophic nitrite-oxidizing bacteria (NOB).
NOB are the main biological source of nitrate, an important nitrogen source for many plants and microorganisms and an electron acceptor used by many microbes under anoxic conditions. Additionally, NOB have a strong impact on marine carbon cycling (2). Recently, surprising discoveries have been made in NOB-related research, demonstrating alternative energy metabolisms, such as the oxidation of hydrogen, sulfide, formate, and other organic compounds in organisms previously described as obligate nitrifiers (35). Furthermore, a novel “reciprocal feeding” interaction of NOB from the genus Nitrospira with ammonia oxidizers was described, where the NOB initiate nitrification by releasing ammonia from urea or cyanate (4, 6). Another surprise was the discovery of photolithoautotrophic NOB that use nitrite as an electron donor for anoxygenic photosynthesis (7) and most likely evolved independently of the chemolithoautotrophic NOB (8). For decades, a core paradigm of nitrification research stated that ammonia and nitrite oxidation are always catalyzed by distinct organisms, which cooperate by cross-feeding. This long-standing opinion was contradicted by the discovery of complete nitrifiers (comammox organisms) in the NOB genus Nitrospira, which perform both steps of nitrification (9, 10). All NOB known until recently belong to the classes Alpha- and Gammaproteobacteria, the phylum Nitrospirae, or the phylum Nitrospinae (1113). The known phylogenetic diversity of NOB has been now expanded by the description of several new NOB lineages: the genus Nitrolancea in the Chloroflexi (14), the candidate genus “Candidatus Nitromaritima” in the Nitrospinae (15), and the candidate genus “Candidatus Nitrotoga” in the Betaproteobacteria, family Gallionellaceae (16).
Past research demonstrated that Nitrospira bacteria are the major NOB in many WWTPs (17, 18). However, “Candidatus Nitrotoga” has recently been recognized as another widely distributed and sometimes predominant group of NOB in WWTPs (1921). Other known habitats of “Ca. Nitrotoga” include soil, sediment, tap water and recirculation aquaculture biofilms, caves, and subglacial lake ecosystems (16, 2226). Despite their importance, little is known about the microbiology of “Ca. Nitrotoga.” The first representative, “Ca. Nitrotoga arctica,” was enriched from Siberian permafrost soil (16). This organism and “Ca. Nitrotoga” members enriched from activated sludge (21) or eelgrass sediment (22) are adapted to cold temperatures. Moreover, a slightly acidic pH (5.7 to 6.8) and elevated nitrite loading were reported to favor growth of “Ca. Nitrotoga” over Nitrospira (24, 25, 27). In addition, the kinetics of nitrite oxidation were studied using enriched “Ca. Nitrotoga” members (22, 28). Further characterization of “Ca. Nitrotoga,” including the nature of its nitrite-oxidizing enzyme and potential for alternative energy metabolisms, has been hampered by the lack of any pure culture or genome sequence from this genus.
In this study, we obtained the first “Ca. Nitrotoga” isolate, characterized its key physiological properties, and analyzed its genetic repertoire based on the fully sequenced genome. The new strain, which has been isolated from a municipal WWTP, shows remarkably different physiological adaptations than the previously described “Ca. Nitrotoga” enrichments. Phylogenetic analysis of its nitrite oxidoreductase (NXR), the key enzyme for nitrite oxidation, suggests that the evolutionary history of NOB is more complex than previously assumed and indicates that a surprising diversity of yet undiscovered bacterial and archaeal nitrite oxidizers may exist in nature.


Isolation of a new “Ca. Nitrotoga” species.

After inoculation of mineral medium (3) containing nitrite with nitrifying activated sludge from a municipal wastewater treatment plant (WWTP) and repeated feeding with nitrite, a nitrite-oxidizing primary enrichment culture was obtained. An initial analysis of the culture by 16S rRNA-targeted fluorescence in situ hybridization (FISH) revealed the presence of Nitrospira, “Ca. Nitrotoga,” and other bacteria. Aliquots of this culture were regularly diluted in fresh nitrite-containing medium and incubated to further enrich the NOB. After the third dilution and transfer step, planktonic “Ca. Nitrotoga” cells were still detected by FISH in the culture, whereas Nitrospira cells were not found. Nitrospira might still have been present in abundances below the detection limit of FISH of approximately 104 target cells per ml (29). The cause of the prevalence of “Ca. Nitrotoga” at this stage of enrichment remains unknown. In addition, this secondary enrichment contained other bacteria that were probably feeding on organic compounds produced by the autotrophic NOB.
Since all further attempts to purify “Ca. Nitrotoga” in liquid culture were unsuccessful, the capability of this nitrite oxidizer to grow on solid medium containing nitrite was tested. Except for some Nitrobacter strains (30) and Nitrolancea hollandica (14), no pure culture of NOB has been grown on solid media. NOB streaked onto plates might be inhibited by ambient oxygen (31) or by organic compounds in commonly used solidifying agents (32). Inhibition could also be caused by H2O2 that is formed when medium containing agar (or agarose) and phosphate is autoclaved (33). No growth of “Ca. Nitrotoga” was observed after streaking aliquots of the secondary enrichment onto plaque agarose plates that had been autoclaved in the presence of phosphate and on media containing Noble agar or sieve agarose (with phosphate added before or after autoclaving). In contrast, small (<1 mm), light brown colonies were obtained after incubation for 1 month on plaque agarose medium prepared by the addition of phosphate after autoclaving. Direct Sanger sequencing of 16S rRNA genes PCR amplified from these colonies confirmed that the colonies consisted of “Ca. Nitrotoga” cells. The obtained 16S rRNA gene sequence was identical to that retrieved from subsequent liquid cultures (see below and Fig. 1). Thus, selection of a suitable solidifying agent and reduction of H2O2 formation in the medium were the key prerequisites for growing “Ca. Nitrotoga” on plates. A single colony was then restreaked onto new plates, and cells were finally transferred into liquid medium containing nitrite. Subsequent purity checks (see Materials and Methods) confirmed the absence of any other organism in the culture.
FIG 1 
FIG 1 Phylogenetic affiliation of “Candidatus Nitrotoga fabula.” The consensus tree, which is based on 16S rRNA gene sequences of cultured and uncultured members of the candidate genus “Nitrotoga” shows the position of the “Ca. Nitrotoga fabula” isolate (indicated in orange) in this genus. Other cultured (enriched) “Ca. Nitrotoga” strains are indicated by boldface type. Pie charts indicate statistical support of branches based on maximum likelihood (RAxML; 1,000 bootstrap iterations) and neighbor joining (NJ) (1,000 bootstrap iterations). For PhyML, no bootstrap analysis was performed and gray indicates the presence of a branch. Bar, 0.01 estimated substitutions per nucleotide.
Phylogenetic analysis of 16S rRNA genes revealed a close affiliation of the obtained “Ca. Nitrotoga” isolate with all other enriched “Ca. Nitrotoga” strains and various environmental sequences (Fig. 1). The highest 16S rRNA gene sequence identity shared by the new isolate and a previously enriched “Ca. Nitrotoga” member was 98.63% with “Ca. Nitrotoga” sp. strain HW29 (25). As this value is below the threshold of 98.7 to 99% used to differentiate species (34) and the obtained isolate showed distinct physiological properties (see below), we propose that this organism represents a separate species within the candidate genus “Ca. Nitrotoga.”
The new “Ca. Nitrotoga” isolate had a peculiar bean-shaped morphology, and the periplasmic space was not enlarged as much as previously described for “Ca. Nitrotoga” cells (16, 21, 22) (Fig. 2). Because of the characteristic morphology, we propose the name “Candidatus Nitrotoga fabula KNB” (“small bean,” strain designation KNB for the WWTP in Klosterneuburg, Austria) for the new isolate.
FIG 2 
FIG 2 Morphology of “Ca. Nitrotoga fabula.” (A) Pure culture of “Ca. Nitrotoga fabula” visualized by FISH with the “Ca. Nitrotoga”-specific probe Ntoga122 (red) and by DAPI staining (blue). Bar, 2 µm. (B) Scanning electron micrograph imaged after chemical fixation (bar, 2 µm). (C and D) Transmission electron micrographs (after cryopreservation [C] and after chemical fixation [D]; bars, 0.5 µm). Black arrows indicate the periplasmic space.

Physiological characterization of “Ca. Nitrotoga fabula” in comparison to previous “Ca. Nitrotoga” enrichments and other NOB.

The nitrite-oxidizing activity of “Ca. Nitrotoga fabula” had its temperature optimum at 24 to 28°C and was poor below 20°C (Fig. 3A). This preference for elevated temperatures was unexpected, because all characterized enriched “Ca. Nitrotoga” members prefer lower temperatures or at least remain active under cold conditions (Table 1). The temperature optimum of “Ca. Nitrotoga fabula” rather resembles that of some NOB in the genus Nitrospira also isolated from WWTPs (32). However, it is noteworthy that uncultured “Ca. Nitrotoga” in WWTPs showed activity over a broad range of temperatures from 4 to 27°C (19) (Table 1). Thus, “Ca. Nitrotoga” members cover a broad temperature range, and not all species are adapted to low temperature, as was previously assumed for this genus.
FIG 3 
FIG 3 Temperature and pH optima for the nitrite-oxidizing activity of “Ca. Nitrotoga fabula.” (A) Mean nitrite oxidation rates during 48 h of incubation at different temperatures. (B) Mean nitrite oxidation rates during 21 h of incubation at different pHs. (A and B) Values are means ± standard deviations (error bars) for three biological replicates. If not visible, error bars are smaller than data points. Values that are significantly different by Welch’s t test are indicated by bars and asterisks as follows: **, P < 0.01; ***, P < 0.001.
TABLE 1 Physiological characteristics of isolated or enriched NOB in the candidate genus “Candidatus Nitrotoga”a
Ca. Nitrotoga” strainTemp optimum (°C)pH optimumNitrite concn
tolerated (mM)
Nitrate concn
tolerated (mM)
Km(app) NO2
Ca. Nitrotoga fabula”
KNB (isolate)
24 to 28 (poor activity
at <20)
7.1 to 7.6Max. concn ND
(activity at 1 to 30)
≤2589.3 ± 3.9
Ca. Nitrotoga arctica”
6680 (enrichment)b
10ND (cultured at
7.4 to 7.6)
<1.2ND58 ± 28
Ca. Nitrotoga” sp. strain
HAM-1 (enrichment)c
ND (cultured at 10
and 17)
ND (cultured at
7.4 to 7.6)
Max. concn ND
(cultured at 0.3)
Ca. Nitrotoga” sp. strain
AM1 (enrichment)d
16ND (cultured at
8.0 to 8.3)
Max. concn ND
(cultured at 0.7 to 2.6)
ND24.7 ± 9.8
Ca. Nitrotoga” sp. strain
HW29 (enrichment)e
22 (40% of max.
activity at 10)
Uncultured “Ca. Nitrotoga”
in WWTPsf
Activity at 4 to 27NDActivity at 0.1 to 10NDND
Data for uncultured “Ca. Nitrotoga” in activated sludge are listed for comparison. Abbreviations: max., maximum; ND, not determined.
Data from references 16 and 28.
Data from reference 21.
Data from reference 22.
Data from reference 25.
Data from reference 19.
The pH optimum of “Ca. Nitrotoga fabula” was between 7.1 and 7.6, and activity decreased at more acidic or alkaline conditions (Fig. 3B). Similar to temperature, adaptation to pH varies among “Ca. Nitrotoga” members (Table 1). For example, “Ca. Nitrotoga” sp. strain HW29 oxidized nitrite most actively at pH 6.8 and retained as much as 75% of its maximal activity at pH 6.1 (25), whereas “Ca. Nitrotoga fabula” lost approximately 75% of its maximal activity already at pH 6.6 (Fig. 3B). “Ca. Nitrotoga fabula” showed no lag phase of its nitrite-oxidizing activity even with 30 mM nitrite in the medium (see Fig. S1A in the supplemental material), and thus, it tolerated much higher nitrite concentrations than other, enriched “Ca. Nitrotoga” members (Table 1). A high tolerance to nitrite was also reported for Nitrospira defluvii (maximum 25 mM) (35) and Nitrolancea hollandica (75 mM), two other NOB isolated from activated sludge (14, 32). Little is known about the nitrate tolerance of “Ca. Nitrotoga.” Nitrite oxidation by “Ca. Nitrotoga fabula” remained completely inhibited in the presence of >25 mM nitrate even after 1 year of incubation (Fig. S1B).
Nitrite oxidation by “Ca. Nitrotoga fabula” followed Michaelis-Menten kinetics (Fig. 4 and Fig. S2), with a mean apparent half-saturation constant of Km(app) = 89.3 ± 3.9 µM (standard deviation [SD]) nitrite. The calculated mean maximum oxidation rate of nitrite (Vmax) was 27.6 ± 8.4 µmol of nitrite (mg of protein ⋅ h)−1 (Fig. 4 and Fig. S2). The measured Km(app)(NO2) of “Ca. Nitrotoga fabula” was higher (but still in the same order of magnitude) than values reported for “Ca. Nitrotoga” enrichments from soil and sediment (Table 1). The slightly poorer affinity for nitrite of “Ca. Nitrotoga fabula” may reflect adaptation to different habitats. However, in enrichment cultures, the accompanying organisms may also respire oxygen or use nitrite (e.g., for denitrification) and thus affect affinity measurements based on respirometry (28) or nitrite consumption (22). In either case, the affinity of the NOB can be overestimated in enrichment cultures. Thus, comparison of results obtained by analyses of an isolate and of enrichment cultures must be interpreted with caution. In comparison to other NOB, the affinity for nitrite of “Ca. Nitrotoga” is moderate (see Table S1 in the supplemental material). In particular, Nitrospira with a significantly higher affinity (Table S1) may outcompete “Ca. Nitrotoga” in oligotrophic habitats and in continuously operated WWTPs (which resemble chemostats) where ambient nitrite concentrations are low.
FIG 4 
FIG 4 Nitrite oxidation kinetics of “Ca. Nitrotoga fabula.” Nitrite oxidation rates were calculated from microsensor measurements of nitrite-dependent O2 consumption. The curve indicates the best fit of the data to the Michaelis-Menten kinetic equation. The protein concentration used to calculate Vmax was 46.1 mg/liter. The experiment was performed with biomass concentrated by centrifugation. Data from three additional biological replicates are shown in Fig. S2 in the supplemental material.
Altogether, adaptations of NOB in the genus “Ca. Nitrotoga” to a broad range of conditions (Table 1) likely reflect the wide distribution of this genus in natural and engineered ecosystems.

Genomic characterization of “Ca. Nitrotoga fabula.”

The genome of the “Ca. Nitrotoga fabula” isolate was completely reconstructed and closed by Illumina and nanopore sequencing (Table S2 and Fig. S3). The chromosome comprises 2,609,426 bp, has an average G+C content of 50.14%, and contains 2,609 coding sequences (CDS). Core metabolic pathways of “Ca. Nitrotoga fabula” were reconstructed from the genomic data (Fig. 5 and Table S4). Interestingly, “Ca. Nitrotoga fabula” possesses a plasmid that has a size of 5,404 bp and contains six CDS (Tables S2 and S3). Its average G+C content of 63.55% differs drastically from the G+C content of the chromosome, indicating horizontal acquisition of the plasmid. The high similarity of all six CDS to homologs in Alpha-, Beta-, and Gammaproteobacteria (Table S3) suggests a proteobacterial plasmid donor. Plasmids are a rare feature in NOB reported so far only for Nitrobacter (36, 37). The plasmid of “Ca. Nitrotoga fabula” encodes two hypothetical proteins, a putative transcriptional regulator, a quaternary ammonium compound resistance protein (EmrE), a putative relaxase, and a putative replication initiation protein (Table S3). The latter two are likely involved in plasmid acquisition and replication, respectively. EmrE might be beneficial for life in activated sludge (see below). The plasmid and the capability of “Ca. Nitrotoga fabula” to grow on solid media could facilitate the development of a vector and a transformant selection system for using “Ca. Nitrotoga fabula” as a genetically tractable model nitrite oxidizer. To date, no genetic system has been established for any NOB.
FIG 5 
FIG 5 Cell metabolic cartoon constructed from the annotation of the “Ca. Nitrotoga fabula” genome. Enzyme complexes of the electron transport chain are labeled with Roman numerals. Table S4 contains further information on the depicted enzymes and pathways. Abbreviations: ACIII, alternative complex III; AnoI/R, acyl-homoserine-lactone synthase/response regulator; CA, carbonic anhydrase; CAT, catalase; CLD, chlorite dismutase; CoA, coenzyme A; CRISPR, clustered regularly interspaced short palindromic repeats; CysH, adenylyl-sulfate reductase; CysND, sulfate adenylyltransferase; HOX, bidirectional group 3d [NiFe] hydrogenase; 2-Hydroxyethyl-ThPP, 2-hydroxyethyl thiamine diphosphate MSC, mechanosensitive channel; NAS, assimilatory nitrite reductase; NirK, nitrite reductase; NXR, nitrite oxidoreductase; RND transporter, resistance-nodulation-cell division transporter; QAC, quaternary ammonium compound; SOD, superoxide dismutase; SIR, assimilatory sulfite reductase; Sor, sulfite:cytochrome c oxidoreductase; TAT, twin-arginine translocation; TCA cycle, tricarboxylic acid cycle; Sec, secretion.

Nitrite oxidation and nitrite oxidoreductase phylogeny.

Nitrite oxidoreductase (NXR), the key enzyme for nitrite oxidation, belongs to the type II dimethyl sulfoxide (DMSO) reductase family of molybdopterin cofactor-binding enzymes (38, 39). The catalytic alpha subunit (NxrA) of known NXRs contains the Mo cofactor and one Fe-S cluster. It is associated with the beta subunit NxrB, which contains four Fe-S clusters. NxrB likely transfers electrons derived from nitrite to the gamma subunit NxrC or directly to the respiratory chain (39). NXR was reported to be a membrane-associated enzyme (3941). The proposed membrane anchor is NxrC, which probably binds one or two heme groups and may thus also be involved in electron transfer (39). The three known types of NXR differ in their cellular localization and phylogenetic affiliation (39). In two groups, NxrA and NxrB face the cytoplasmic side of the cell membrane (8, 41). These NXRs are closely related to membrane-bound, cytoplasmically oriented nitrate reductases (NARs) (Fig. 6). One type is found in Nitrobacter, Nitrococcus, and Nitrolancea, and the second type is found in the phototrophic NOB Thiocapsa strain KS1 (5, 8, 14, 38) (Fig. 6). In the third group, NxrA and NxrB are oriented toward the periplasmic space. This type occurs in Nitrospira, Nitrospina, and in anaerobic ammonium oxidizers (anammox organisms) and is phylogenetically distinct from the cytoplasmic NXRs (13, 39, 40) (Fig. 6). In anammox organisms, NXR is localized in the anammoxosome instead of the periplasm (42).
FIG 6 
FIG 6 Phylogeny of NxrA from “Ca. Nitrotoga fabula” and related proteins. Consensus tree showing the alpha subunits of selected enzymes from the type II DMSO reductase family. Confirmed and putative (put.) NxrA and NarG proteins are indicated. Organisms or enrichment cultures with an observed nitrite-oxidizing phenotype are shown in orange, those with an observed nitrate-reducing phenotype are shown in purple. Pie charts indicate statistical support based on maximum likelihood (ML) (1,000 bootstrap iterations) and Bayesian inference (BI) (posterior probability, 10 independent chains). Numbers in wedges indicate the numbers of taxa. Abbreviations: ClrA, chlorate reductase; DdhA, dimethylsulfide dehydrogenase; EbdA, ethylbenzene dehydrogenase; PcrA, perchlorate reductase; SerA, selenate reductase. Bar, 0.01 estimated substitutions per residue.
Consistent with its growth on nitrite as the sole energy source and electron donor, “Ca. Nitrotoga fabula” encodes NXR (Fig. 5, Fig. S3, and Table S4). The genome contains two identical loci coding for NxrA, NxrB, a putative NxrC, and a putative chaperone (Fig. S3 and Table S4). No other nxr genes were identified. NxrA and NxrB of “Ca. Nitrotoga fabula” contain the conserved binding sites for the Mo cofactor and the Fe-S clusters found also in the respective homologs of Nitrospira defluvii (39) with only few differences. In NxrA, the Mo binding site has the sequence pattern Y-4x-D-11x-QM instead of Y-4x-D-11x-QN as in N. defluvii. In NxrB of “Ca. Nitrotoga fabula,” the binding site of Fe-S cluster IV contains cysteine at the position homologous to Asp45 of N. defluvii and lacks an insertion of eight residues that is found in N. defluvii (39). NxrC shows only low similarity to gamma subunits of other type II DMSO reductase-like enzymes. It contains a predicted heme-binding site but no transmembrane helix, indicating that the NXR of “Ca. Nitrotoga fabula” may be soluble or interacts with another membrane-bound protein, as was also discussed for Nitrospina gracilis (13). NxrA contains an N-terminal signal peptide for protein export via the twin-arginine protein translocation mechanism, and NxrC contains an N-terminal signal peptide for translocation via the Sec pathway, suggesting that the NXR of “Ca. Nitrotoga fabula” is located in the periplasmic space (Fig. 5). NxrB lacks any translocation signal but may be cotranslocated with NxrA as proposed for the periplasmic NXRs of Nitrospira and Nitrospina (13, 39). A periplasmic NXR should be energetically advantageous, because nitrite oxidation outside the cell releases protons into the periplasm and may contribute directly to proton motive force (PMF) (39) (Fig. 5). This feature likely helps “Ca. Nitrotoga” compete with cooccurring NOB harboring a cytoplasmic NXR.
Intriguingly, phylogenetic analysis of the catalytic NxrA subunit revealed that the NXR of “Ca. Nitrotoga fabula” is not closely related to the other known NXR forms. Instead, it belongs to a distinct “sister clade” of the lineage containing the periplasmic NXRs of Nitrospira, Nitrospina, and anammox (Fig. 6). Some of the proteins affiliated with NxrA of “Ca. Nitrotoga fabula” are catalytic subunits of putative NARs (NarG) from phylogenetically diverse bacteria and archaea, which are known nitrate reducers (Fig. 6). Only recently, the enzyme of Hydrogenobacter thermophilus has been functionally characterized as a periplasmically oriented, membrane-bound NAR (43). The affiliation of NXR from “Ca. Nitrotoga fabula” with this clade demonstrates that enzymes in this group are capable of nitrite oxidation. Since other NXRs are bidirectional enzymes that oxidize nitrite and also reduce nitrate (4, 5, 44), it is conceivable that known nitrate-reducing members of this clade could also oxidize nitrite for detoxification or even for energy conservation under permissive conditions. An additional requirement for nitrite oxidation would be suitable electron carriers, such as high-potential cytochrome c (cyt. c), which accept the electrons derived by NXR from nitrite. To our knowledge, except for “Ca. Nitrotoga fabula,” none of the cultured organisms possessing enzymes in this NXR/NAR clade has systematically been tested for a nitrite-oxidizing phenotype. Moreover, the clade contains proteins from highly diverse, uncultured, and physiologically uncharacterized organisms (Fig. 6) that might be novel nitrite oxidizers if they also possess high-potential electron carriers. According to this assumption, nitrite oxidation might occur within the domain Archaea (Fig. 6). Recently, we sequenced a joint metagenome from pooled DNA from early stage nitrifying enrichments, which had been established at 75°C from a hot spring in Iceland (Text S1). Nitrite oxidation had been observed in several of these cultures. The only nxr-like genes found in the assembly were binned into a metagenome-assembled genome of a crenarcheon, which was remotely related to the genus Ignisphaera (family Desulfurococcaceae) (Fig. S4). Intriguingly, its putative NxrA fell into the same clade as the NxrA of “Ca. Nitrotoga fabula.” It grouped with the NxrA/NarG of “Candidatus Caldiarchaeum subterraneum” (phylum “Aigarchaeota”), an uncultured and phenotypically uncharacterized thermophilic archaeon (Fig. 6). The absence of unambiguously detected, canonical NOB from the metagenomic data set and the presence of archaea possessing a putative NXR is highly conspicuous and deserves further investigation.
Previous analyses suggested that NXR independently evolved at least three times within the type II DMSO reductase family, leading to the aforementioned three types of cytoplasmic and periplasmic NXRs (8, 39). The distinct phylogenetic position of the novel NXR of “Ca. Nitrotoga fabula” indicates an even more complex evolutionary history of nitrite oxidation. Functional data for the enzymes in this clade are too sparse to assess whether nitrite oxidation may be an ancestral feature of this lineage, or more likely a secondary adaptation found in “Ca. Nitrotoga” (and possibly additional organisms) with the remaining proteins being strict NARs. However, it is remarkable that the clade shares a common ancestor with the Nitrospira/Nitrospina/anammox enzymes, which are exclusively NXRs (Fig. 6). It also remains unclear whether this type of NXR evolved in “Ca. Nitrotoga” or was acquired through horizontal gene transfer by an ancestor of this genus.

Central energy and carbon metabolism.

In NOB, electrons derived from nitrite are transferred from NXR to cyt. c and then to the terminal oxidase (cyt. c oxidase; complex IV) for aerobic respiration (Fig. 5). The genome of “Ca. Nitrotoga fabula” encodes several c-type cytochromes and a predicted high-affinity, proton-pumping heme-copper cyt. c oxidase of the cbb3 type (Table S4). The conserved energy is used for ATP synthesis by a canonical F1Fo ATPase (complex V) (Fig. 5 and Table S4). In addition, “Ca. Nitrotoga fabula” possesses a canonical NADH dehydrogenase (complex I) and the complete oxidative tricarboxylic acid (TCA) cycle, including a four-subunit succinate dehydrogenase complex (complex II) (Fig. 5 and Table S4). A canonical quinol:cytochrome c oxidoreductase (complex III) is lacking, but “Ca. Nitrotoga fabula” carries genes encoding an alternative complex III (ACIII) (45) that is highly similar to ACIII of other Gallionellaceae members (46). Thus, “Ca. Nitrotoga fabula” possesses a complete electron transport chain for respiration using inorganic low-potential electron donors such as H2 (see below) or organic compounds. For example, glycogen deposits may serve as an energy source for cell maintenance during starvation (Fig. 5 and Table S4). However, “Ca. Nitrotoga fabula” appears to lack genes encoding components in the uptake and utilization of formate, pyruvate, and acetate, which can be used as carbon and/or energy sources by several other NOB (4, 18, 47, 48). A transporter for branched amino acids may enable their use as organic sources of energy, carbon and nitrogen, or directly as protein building blocks (Fig. 5). “Ca. Nitrotoga fabula” can also assimilate nitrogen from ammonium and nitrite (Table S4), but in contrast to some other NOB (4, 6), it lacks any known genes for utilizing urea or cyanate.
When nitrite is the sole electron donor, reductants for autotrophic CO2 fixation must be provided by reverse electron transport. Unlike Nitrospira, “Ca. Nitrotoga fabula” lacks multiple copies of complexes I and III that might channel electrons in opposite directions (4, 39). Thus, we assume that these single complexes of “Ca. Nitrotoga fabula” are bidirectional and consume PMF for reverse electron transport (Fig. 5). “Ca. Nitrotoga fabula” carries genes encoding all the components of the complete Calvin-Benson-Bassham (CBB) cycle for CO2 fixation, including two divergent copies of the small (37% amino acid identity) and large (56% identity) subunits of type I ribulose-1,5-bisphosphate carboxylase/oxygenase (RuBisCO). Other NOB using the CBB cycle are Nitrobacter, Nitrococcus, and Nitrolancea (5, 14, 49). In contrast, Nitrospira and Nitrospina utilize the more oxygen-sensitive reductive TCA cycle (13, 39). Hence, “Ca. Nitrotoga” might be more resistant to high dissolved oxygen (DO) concentrations and could have a competitive advantage over Nitrospira in strongly aerated activated sludge tanks. Based on its predicted high-affinity terminal oxidase (see above), “Ca. Nitrotoga fabula” could also cope with low-DO conditions that occur, for example, in simultaneously nitrifying and denitrifying bioreactors. This may explain the observed presence of “Ca. Nitrotoga” in a low-DO nitrifying bioreactor where it cooccurred with Nitrospira (50), which can also oxidize nitrite at low DO concentrations (51, 52).

Alternative energy metabolisms.

The recent discovery that some Nitrospira grow chemolithoautotrophically by aerobic hydrogen oxidation was unexpected, because nitrifiers had been regarded as metabolically restricted organisms whose energy metabolism is intimately linked to the nitrogen cycle (3). Interestingly, “Ca. Nitrotoga fabula” harbors a complete set of genes encoding a group 3d NAD-coupled [NiFe] hydrogenase and accessory proteins (Fig. S3 and Table S4) (53). The enzymes in this group are cytosolic bidirectional hydrogenases and can be oxygen tolerant (54). The hydrogenase could enable “Ca. Nitrotoga fabula” to use H2 as an energy source and electron donor for aerobic growth and, if NXR works reversibly, for anaerobic respiration with nitrate as electron acceptor. Both activities were observed for Nitrospira moscoviensis, although growth occurred only in oxic incubations (3, 12). Hydrogenases occur in various NOB (3), and hydrogen oxidation as an alternative energy metabolism has several advantages for these organisms. First, it can help NOB survive nitrite-depleted conditions. Second, electrons derived from H2 can be used for CO2 fixation without reverse electron transport, saving energy for other cellular functions. Finally, it may enable NOB to colonize niches independent of nitrification. A source of H2 could be fermenting heterotrophs living nearby in anoxic niches in soils, sediments, biofilms, and flocs (55).
Ca. Nitrotoga fabula” also carries genes encoding a periplasmic sulfite:cyt. c oxidoreductase (Fig. 5 and Table S4), which may allow it to use sulfite as an energy source and electron donor. Recently, the participation of NOB in sulfur cycling was demonstrated for Nitrococcus that oxidized sulfide in the presence of O2 (5).

Stress response, defense, and cell-cell communication.

Contrasting their aerobic metabolism, several NOB and also comammox organisms lack catalase, superoxide dismutase, or both (9, 13, 39). “Ca. Nitrotoga fabula” possesses both enzymes (Fig. 5 and Table S4) but apparently was nevertheless inhibited by the amount of H2O2 formed during the preparation of solid media with phosphate (see above).
Wastewater contains many potentially toxic compounds. Accordingly, the genome of “Ca. Nitrotoga fabula” encodes various resistance and detoxification mechanisms, including efflux systems for heavy metals and organic solvents, arsenate reductase, and chlorite dismutase (Fig. 5 and Table S4). Quaternary ammonium compounds (QAC) are widely used as disinfectants and are ingredients in cosmetics and household products. In addition to the emrE gene on the plasmid (see above), “Ca. Nitrotoga fabula” has another QAC resistance gene (sugE) on the chromosome. QAC resistance is not a common feature of NOB isolated from WWTPs. While the genome of Nitrospira defluvii encodes SugE, both Nitrospira japonica NJ1 and Nitrospira strain ND1 (56) lack QAC resistance genes. The sensitivity of NOB to QAC and other harmful compounds has hardly been studied, but it could be an important factor determining the distribution and abundance of different NOB in sewage treatment systems.
Ca. Nitrotoga fabula” possesses a LuxI/LuxR-type quorum-sensing (QS) system that is similar to the AnoI/AnoR system of Acinetobacter nosocomialis (57) (56% amino acid sequence identity to AnoI and 46% identity to AnoR). QS systems have also been identified in Nitrobacter and Nitrospira (56, 58). In Nitrobacter, QS has been linked to the production and consumption of nitrogen oxides (59). Further functions of QS in NOB await investigation, and it will be exciting to see whether QS plays similar or different roles in phylogenetically diverse NOB, including “Ca. Nitrotoga.”

Description of “Candidatus Nitrotoga fabula”.

Fabula (L. fem. noun, small bean, referring to the characteristic bean-shaped morphology of the cells).
Cells are Gram-negative short curved rods with a length of approximately 1 µm and width of approximately 0.5 µm. “Ca. Nitrotoga fabula” grows planktonically but forms loose flocs at high cell density. Nonmotile. Aerobic chemolithoautotrophic nitrite oxidizer that uses CO2 as the sole carbon source. Temperature optimum of 24 to 28°C, pH optimum of 7.1 to 7.6. Nitrite oxidation was observed up to 30 mM nitrite (higher concentrations not tested) and below 30 mM nitrate. Grows in mineral liquid and on solid (plaque agarose autoclaved without phosphate) media containing nitrite. The genome consists of a single chromosome and a plasmid. The G+C content of the DNA is 50.14 mol% (chromosome) and 63.55 mol% (plasmid).
The “Ca. Nitrotoga fabula” KNB strain was isolated from activated sludge of the municipal wastewater treatment plant in Klosterneuburg, Austria. The strain is available from the authors upon request.


The physiological and genomic characterization of the first “Ca. Nitrotoga” isolate has revealed potential alternative energy metabolisms and a broader spectrum of physiological adaptations in this genus than previously assumed. Like Nitrospira, “Ca. Nitrotoga” members can be versatile NOB whose metabolic flexibility may explain their competitive success in dynamic environments such as WWTPs. However, fundamental differences between “Ca. Nitrotoga” and Nitrospira include the affinity for nitrite (Table S1), as well as the resistance of “Ca. Nitrotoga” to higher oxygen levels according to the genetic inventory and growth on plates of “Ca. Nitrotoga fabula.” Previous studies showed that multiple factors, including the concentrations of DO and nitrite, temperature, and pH, influence the community composition of NOB (21, 25, 50, 51, 60, 61). Further research is needed to understand which conditions in engineered and natural ecosystems allow the coexistence of “Ca. Nitrotoga” with Nitrospira or other NOB and which factors lead to their competitive exclusion. Intriguingly, the phylogenetic affiliation of the novel NXR of “Ca. Nitrotoga” with enzymes from uncharacterized microorganisms indicates that the diversity of nitrite oxidizers in nature might be much larger than currently anticipated.


Sampling and cultivation conditions.

Activated sludge from the combined nitrification/denitrification tank (intermittently aerated; maximum dissolved oxygen [DO] concentration of 2.5 mg/liter) of the municipal wastewater treatment plant (WWTP) in Klosterneuburg, Austria, was sampled in January 2014. The sludge was diluted 1:3,000 in mineral medium that was prepared as described elsewhere (3) and amended with 3 µg Na2SeO3⋅5H2O and 4 µg Na2WO4⋅2H2O per liter. Diluted sludge (150 ml) was inoculated in 300-ml Erlenmeyer flasks that were loosely closed with aluminum caps, supplied with 1 mM NaNO2, and incubated at room temperature in darkness and without agitation. Nitrite consumption was regularly monitored by using nitrite-nitrate test strips (Merckoquant; Merck). Upon depletion of nitrite, the cultures were fed with 1 mM NaNO2. Aliquots of the enrichments were subcultured into fresh medium (dilution factor of 1:200) in intervals of 3 to 8 weeks. After the second transfer, the cultures were kept in 100-ml borosilicate bottles filled with 40 ml medium and closed with plastic lids.
Solid mineral media containing nitrite were prepared with 1% (wt/vol) Noble agar (catalog no. 214220; Difco), sieve 3:1 agarose (catalog no. 850091; Biozym), or plaque agarose (catalog no. 840100; Biozym). The pH of the medium was adjusted to pH 7.8 either by adding KH2PO4 prior to the addition of solidifying agent and autoclaving or by adding sterile filtered KH2PO4 of pH 8 after autoclaving. Aliquots (5 to 10 µl) of 1:100 diluted culture were streaked onto the solid media and incubated at room temperature in darkness for several weeks. Grown colonies were restreaked onto solid medium, and single colonies were finally inoculated into liquid mineral medium. Culture aliquots were cryopreserved in mineral medium containing 10% (vol/vol) dimethyl sulfoxide (DMSO) (62).

Assessment of culture purity.

The nitrite-oxidizing bacterial (NOB) community composition in liquid enrichment cultures was monitored by rRNA-targeted fluorescence in situ hybridization (FISH) after cell fixation in formalin according to standard protocols (63). The oligonucleotide probes applied were Ntspa662 specific for the genus Nitrospira (18), Ntoga122 specific for the candidate genus “Nitrotoga” (19), probes EUB338-I to -III that detect most bacteria (64, 65), and NON338 as a control for nonspecific probe binding (66). The probes were 5′ and 3′ doubly labeled with the fluorochromes Fluos, Cy3, and Cy5 and used in combination with the unlabeled competitor oligonucleotides of Ntspa662 and Ntoga122, respectively (18, 19). FISH was combined with nonspecific fluorescent labeling of all cells by 4′,6′-diamidino-2-phenylindole (DAPI). Fluorescence micrographs were recorded using an epifluorescence microscope (Zeiss Axio Imager M2 with AxioCam 506 Mono). The purity of the “Ca. Nitrotoga fabula” isolate was assessed by the following: (i) FISH and DAPI staining as described above; (ii) inoculation of Luria-Bertani medium, which was diluted 1:10 in mineral medium, to test for heterotrophic contaminants; and (iii) PCR screening of the culture using the primers 8F and 1492R that target the bacterial 16S rRNA gene (17, 67). After purification (QIAquick PCR purification kit; Qiagen), the PCR products were Sanger sequenced (Microsynth, Austria) without cloning. The purity of the isolate was also confirmed by Illumina sequencing (see below) and by the absence of cells with a divergent morphology in electron micrographs (for a detailed description of sample preparation for electron microscopy, see Text S1 in the supplemental material).

Physiological experiments.

Cells from pregrown liquid cultures of “Ca. Nitrotoga fabula” were collected by centrifugation (8,200 × g, 20 min, 20°C). The supernatant was discarded, and the cells were resuspended in fresh mineral medium without nitrite. This procedure was repeated until no nitrite and nitrate was detected in the supernatant. The cells were finally resuspended in fresh mineral medium and served as an inoculum for physiological experiments. All experiments were carried out in biological triplicates. To quantify the nitrite-oxidizing activity, nitrite and nitrate concentrations were measured photometrically as described elsewhere (68, 69). At each time point, samples (0.5 ml) of the incubated cultures were taken, cells were removed by centrifugation (20,100 × g, 10 min, 4°C), and the supernatant was stored at −20°C until chemical measurements were performed. To determine the temperature optimum for activity of “Ca. Nitrotoga fabula,” 100-ml borosilicate glass bottles containing 40 ml medium supplemented with 1 mM NaNO2 were preincubated at the tested temperatures (4 to 46°C). After inoculation with washed cells (see above), the bottles were incubated at the respective temperatures, and the nitrite and nitrate concentrations were quantified after 48 h as described above. To determine the pH optimum for activity of “Ca. Nitrotoga fabula,” mineral medium was supplemented with 5 mM (final concentration) sterile-filtered HEPES (Sigma-Aldrich) after autoclaving. The pH was adjusted to 6.6, 7.1, 7.6, 7.9, and 8.1 by adding 1 N NaOH and remained stable throughout the experiment. Samples for nitrite and nitrate concentration measurements were taken during 3 days of incubation at 28°C.
To determine the nitrite and nitrate tolerance, “Ca. Nitrotoga fabula” cells were incubated in media containing 1 to 30 mM nitrite or 15 to 50 mM nitrate, respectively, at the optimal temperature (28°C). The media containing nitrate were also supplemented with 1 mM nitrite as the substrate. Nitrite oxidation was then monitored for up to 6 weeks (nitrite tolerance) and up to 1 year (nitrate tolerance).
The nitrite oxidation kinetics of “Ca. Nitrotoga fabula” were inferred from instantaneous oxygen uptake measurements in four independent experiments as previously described (70). Nitrite uptake rates were calculated from the measured oxygen uptake rates, and Michaelis-Menten plots of nitrite uptake rates versus nitrite concentration were obtained by fitting a Michaelis-Menten model to the data. Kinetic constants were estimated by nonlinear least-squares regression. For a detailed description of the approach, see Text S1.

DNA extraction, genome sequencing, and genome annotation.

Cells were collected from a liquid “Ca. Nitrotoga fabula” culture, which had been inoculated from a single colony, by centrifugation (8,200 × g, 20 min, 20°C) and frozen at −20°C. Total DNA was extracted according to reference 71 with bead beating for cell disruption at 4 m s−1. The genome of “Ca. Nitrotoga fabula” was sequenced and closed by applying a combination of Illumina and Nanopore technologies (for details of genome sequencing and assembly, please refer to Text S1). The reconstructed genome of “Ca. Nitrotoga fabula” was uploaded to the MicroScope platform (72) for automatic annotation and manual annotation refinement of selected metabolic pathways (39).

Phylogenetic analyses.

Representative full-length 16S rRNA gene sequences classified as “Ca. Nitrotoga” in the SILVA Ref NR 99 database (release 132, 13 December 2017) (73) and the 20 top BLASTN hits (>95% alignment coverage, >98% identity) to the 16S rRNA gene sequence of “Ca. Nitrotoga fabula” were used to calculate phylogenetic trees. The 16S rRNA gene sequences of cultured Gallionella species, and environmental sequences clustering between “Ca. Nitrotoga” and Gallionella, were used as outgroups. Sequences were aligned using SINA (74); the length of analyzed sequences was between 1,361 and 1,528 bp. Trees were calculated using the neighbor-joining implementation in ARB (75) (Jukes-Cantor substitution model; 1,000 bootstrap iterations) and maximum likelihood algorithms implemented in PhyML (76) and RAxML (77) (gamma model of rate heterogeneity and generalized time-reversible [GTR] substitution model; 1,000 bootstrap iterations). A consensus tree was reconstructed using ARB, and branching patterns were compared manually between all calculated trees. NxrA/NarG protein sequences were aligned using mafft-linsi v.7.312 (78) and trimmed using Trimal v1.4.rev15 (79) with option -automated1. The resulting alignment consisting of 1,206 columns was used to calculate trees in IQ-TREE v1.6.2 (80) and PhyloBayes v4.1b (81). IQ-TREE calculations included model prediction by ModelFinder (82), which identified the best-fit model to be LG+R8, and support values for bipartitions were calculated using UFboot2 (83). PhyloBayes calculations were carried out with 10 independent chains of 5,000 generations using the category (CAT)-GTR model; 2,000 generations of each chain were discarded as burn-in, and the remainder were subsampled every third tree and pooled for calculation of posterior probabilities.

Accession number(s).

The genome sequence of “Ca. Nitrotoga fabula” has been deposited in the European Nucleotide Archive (ENA) under project PRJEB26077. The metagenome-assembled genome sequence of the Desulfurococcaceae-related crenarcheon from the thermophilic enrichment has been deposited at NCBI GenBank under project PRJNA461265, accession QFWU00000000.


Daniela Gruber and Norbert Cyran from the Core Facility of Cell Imaging and Ultrastructure Research at the University of Vienna are gratefully acknowledged for help with electron microscopy. We thank A. Giguere and K. D. Kits for assistance with microrespirometry, Andreas Richter for providing samples used to inoculate thermophilic enrichments, and A. Galushko for helpful discussions. We are grateful to M. Ücker for technical assistance.
This study was supported by the Austrian Science Fund (FWF) projects P25231-B21, P27319-B21, P30570-B29, and W 1257 to H.D., FWF project T938-B32 to A.D., the European Research Council Advanced Grant Nitrification Reloaded (NITRICARE) to M.W., a research grant (15510) from VILLUM FONDEN to M.A., the Danish Research Council for Independent Research (DFF) grant 4005-00369 to P.H.N., the Volkswagen Foundation VW-Vorab grant ZN3112 to H.K., the Netherlands Organization for Scientific Research (NWO) grant 863.14.019 to S.L., and the Max Planck Society (N.L.).


This article is a direct contribution from a Fellow of the American Academy of Microbiology. Solicited external reviewers: Willm Martens-Habbena, University of Florida; Daniel Noguera, University of Wisconsin-Madison.

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Information & Contributors


Published In

cover image mBio
Volume 9Number 45 September 2018
eLocator: 10.1128/mbio.01186-18
Editor: Douglas G. Capone, University of Southern California


Received: 29 May 2018
Accepted: 14 June 2018
Published online: 10 July 2018


  1. Archaea
  2. Nitrotoga
  3. activated sludge
  4. ecophysiology
  5. genome analysis
  6. isolate
  7. nitrification
  8. nitrite oxidation



Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Max-Planck-Institute for Marine Microbiology, Bremen, Germany
Hanna Koch
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Present address: Hanna Koch, Department of Microbiology, Radboud University, Nijmegen, The Netherlands.
Sebastian Lücker
Department of Microbiology, Radboud University, Nijmegen, The Netherlands
Christopher J. Sedlacek
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Craig Herbold
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Jasmin Schwarz
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Anne Daebeler
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Anna J. Mueller
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Michael Lukumbuzya
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Stefano Romano
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Nikolaus Leisch
Max-Planck-Institute for Marine Microbiology, Bremen, Germany
Søren Michael Karst
Center for Microbial Communities, Department of Chemistry and Bioscience, Aalborg University, Aalborg, Denmark
Rasmus Kirkegaard
Center for Microbial Communities, Department of Chemistry and Bioscience, Aalborg University, Aalborg, Denmark
Mads Albertsen
Center for Microbial Communities, Department of Chemistry and Bioscience, Aalborg University, Aalborg, Denmark
Per Halkjær Nielsen
Center for Microbial Communities, Department of Chemistry and Bioscience, Aalborg University, Aalborg, Denmark
Michael Wagner
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria
Holger Daims
Division of Microbial Ecology, Department of Microbiology and Ecosystem Science, Research Network “Chemistry meets Microbiology,” University of Vienna, Vienna, Austria


Douglas G. Capone
University of Southern California


Address correspondence to Holger Daims, [email protected].

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