Skip to main content

Advertisement

Niche differentiation in nitrogen metabolism among methanotrophs within an operational taxonomic unit

BMC Microbiology volume 14, Article number: 83 (2014) | Download Citation

Article metrics

Abstract

Background

The currently accepted thesis on nitrogenous fertilizer additions on methane oxidation activity assumes niche partitioning among methanotrophic species, with activity responses to changes in nitrogen content being dependent on the in situ methanotrophic community structure Unfortunately, widely applied tools for microbial community assessment only have a limited phylogenetic resolution mostly restricted to genus level diversity, and not to species level as often mistakenly assumed. As a consequence, intragenus or intraspecies metabolic versatility in nitrogen metabolism was never evaluated nor considered among methanotrophic bacteria as a source of differential responses of methane oxidation to nitrogen amendments.

Results

We demonstrated that fourteen genotypically different Methylomonas strains, thus distinct below the level at which most techniques assign operational taxonomic units (OTU), show a versatile physiology in their nitrogen metabolism. Differential responses, even among strains with identical 16S rRNA or pmoA gene sequences, were observed for production of nitrite and nitrous oxide from nitrate or ammonium, nitrogen fixation and tolerance to high levels of ammonium, nitrate, and hydroxylamine. Overall, reduction of nitrate to nitrite, nitrogen fixation, higher tolerance to ammonium than nitrate and tolerance and assimilation of nitrite were general features.

Conclusions

Differential responses among closely related methanotrophic strains to overcome inhibition and toxicity from high nitrogen loads and assimilation of various nitrogen sources yield competitive fitness advantages to individual methane-oxidizing bacteria. Our observations proved that community structure at the deepest phylogenetic resolution potentially influences in situ functioning.

Background

Methane is a major greenhouse gas, accounting for up to 20-30% of global warming effect [1]. Aerobic methanotrophic bacteria constitute the main microbial methane sink through their ability to derive energy from its oxidation to carbon dioxide using the key enzyme methane monooxygenase [2]. Cultured representatives of this functional guild are phylogenetically positioned within the Gammaproteobacteria (Type I methanotrophs, forming two clades, i.e. Type Ia and Ib), the Alphaproteobacteria (Type II methanotrophs) [3, 4], and the Verrucomicrobia[5]. These methanotrophs appear physiologically diverse, especially in regard to their nitrogen metabolism [6], with strains demonstrating co-metabolic oxidization of ammonia [4], nitrate reduction to nitrite [7], detoxification of hydroxylamine and nitrite to the greenhouse gas nitrous oxide via a multitude of pathways [8–10], and fixation of atmospheric nitrogen [11–14].

The effect of nitrogen, under the form of either ammonium- or nitrate-based fertilizers, on methane fluxes in soils is a widely studied topic of global concern. Unfortunately, available reports are not in agreement, with methanotrophic activity after nitrogen addition either showing no effect, inhibition (by non-specific ionic effects [15], competitive inhibition between methane and ammonia or the formation of toxic intermediates [10, 16]) or stimulation (by relief of nitrogen limitation), resulting in identical or altered associated community composition [17–20]. The currently accepted thesis assumes niche partitioning among methanotrophic species, with methane oxidation activity responses to changes in nitrogen content being dependent on the in situ methanotrophic community structure [19, 21].

Unfortunately, widely applied tools for microbial community assessment, based on short read 16S rRNA gene sequencing techniques or proxies thereof (such as denaturating gradient gel electrophoresis (DGGE) or terminal-restriction fragment length polymorphism (T-RFLP)), only have a limited phylogenetic resolution mostly restricted to genus level diversity [22], and not to species level as often mistakenly assumed. As a consequence, intragenus or intraspecies metabolic versatility in nitrogen metabolism was never evaluated nor considered among methanotrophic bacteria as a source of differential responses of methane oxidation to nitrogen amendments. Nevertheless, we know from other organisms that ecophysiology can be strain-specific, and closely related bacteria can occupy distinct niches [23, 24]. This was for example elaborately demonstrated in Prochlorococcus, with cultured strains having distinct pigmentation, maximum growth rates, metal tolerances, nutrient utilizations and photophysiological characteristics [23]. Also, among methanotrophic genera of the same type (I or II), ammonia co-metabolisation and product inhibition was found to be organism-specific, although in this study it is difficult to ascertain the taxonomic level at which differences occur as only two strains from different genera were tested for each type [10].

We hypothesized that strains within the same methanotrophic genus, thus below the level at which most techniques assign operational taxonomic units (OTU), can demonstrate a large physiological versatility in their nitrogen metabolism. If so, this would make current microbial community structure analyses less suitable for evaluating changes in in situ methanotrophic communities after for example fertilization. To this end, we explored the differential response of various aspects of the nitrogen metabolism within fourteen genotypically distinct members of the genus Methylomonas (Type Ia), including the species M. methanica and M. koyamae. Their tolerance to high ammonium, nitrate, nitrite and hydroxylamine concentrations, their ability to fix nitrogen, and their capacity to produce nitrite and nitrous oxide from nitrate or ammonium were qualitatively evaluated. Methylomonas is a relevant genus for such a comparison, since Methylomonas strains are ubiquitous in nature [4, 7, 25–27] and nitrogenous fertilization was reported to stimulate some of its members in rice field soils [19]. Two non-Methylomonas strains belonging to Type Ib and Type II were included as references.

Results

N2fixation

We screened a strain set of fourteen genotypically distinct Methylomonas strains, one Type Ib strain (Methylococcaceae sp. R-49797) and one Type II strain (Methylosinus sp. R-45379) in batch experiments for their ability to fix dinitrogen gas as sole nitrogen source. Only at low oxygen tension, ten out of the thirteen Methylomonas strains could grow without any nitrogen source except for N2 in the headspace (Table 1), confirming the presence of an oxygen sensitive nitrogenase. Since oxygen became rapidly limiting in the batch setup used, volumes of air equal to the initial volume were injected (up to eight times) to allow further activity and growth of the cultures. Maximum OD600nm values averaged at 0.332 ± 0.122 (start OD600nm values of 0.017 ± 0.019) across strains, while activity was observed with drops in methane and oxygen levels and subsequent increase in CO2 levels (data not shown). No growth or activity was observed for the strains cultivated in parallel in nitrogen-free medium under high oxygen tension, confirming the absence of nitrogenous compounds in the growth medium, which was also demonstrated by colorimetric analysis of nitrate, nitrite and ammonium. To confirm observations, the presence of the nifH gene encoding the Fe protein of nitrogenase was verified. All strains that did not give a nifH gene amplicon were also negative for growth and activity in nitrogen-free medium at high and low oxygen tension.

Table 1 Nitrogen assimilation and tolerance per strain
Full size table

Three tested Methylomonas strains (R-49807, R-45370 and R-45377) were not active and did not grow in nitrogen-free medium under low oxygen tension during the 21-days experiment, although PCR and sequence analyses demonstrated the presence of a nifH gene. M. koyamae R-49807 unexpectedly did not exhibit N2 fixation, although this strain shares a 100% 16S rRNA and a >99% nifH sequence similarity with strains NCIMB 14606T and R-49799 (data not shown), both positive for N2 fixation under low oxygen tension. M. lenta R-45370 and R-45377 typically grew slower than the other strains (one to two-week lag phase in liquid media under optimal conditions). Therefore, it is possible that these strains would fix N2 after longer incubation periods.

Assimilation of nitrate and ammonium and tolerance to high levels

Assimilation of and/or tolerance to high levels of ammonium and nitrate was evaluated, in addition to the influence of general osmotic effects tested with equimolar concentrations of sodium chloride (Table 1). These tests were qualitatively scored based on growth, which was used as a proxy for methane oxidation as both features were shown to correlate (Additional file 1: Figure S1). This experiment was performed in microtiter plates, in which all strains could grow well, even though a more limited gas transfer is expected in such a setup compared with batch experiments due to a lack of mixing. The complete strain panel was able to use both ammonium and nitrate for assimilation and strains could cope in general with a maximum of 40 mM amended nitrogen, except the type II strain, which only tolerated a maximum of 20 mM NO3 −-N (Table 1).

Two M. koyamae strains, R-49799 and NCIMB 14606T, showed a higher tolerance for NH4 +-N, up to 100 mM. Notably, growth at these high ammonium concentrations was not supported for M. koyamae R-49807, showing gene sequence similarity with M. koyamae NCIMB 14606T and M. koyamae R-49799 of 100% for the 16S rRNA gene (Additional file 2: Figure S4, Additional file 3: Table S1) and between 97-100% for the pmoA gene encoding the particulate methane monooxygenase, the key enzyme for methane oxidation (Additional file 4: Figure S5, Additional file 5: Table S2). In addition, out of these three strains only R-49799 exhibited higher sodium chloride tolerance when grown with ammonium as sole nitrogen source over nitrate (150 mM compared with 100 mM). For M. methanica cultures, strains NCIMB 11130T and R-45372 exhibited higher salt tolerance when cultivated with NH4 +-N instead of NO3 −-N. M. methanica R-45364 was salt sensitive regardless of the nitrogen source and demonstrated an equal tolerance to sodium chloride, ammonium and nitrate (≤40 mM). The other M. methanica strains tolerated higher sodium chloride concentrations than equimolar nitrate and ammonium concentrations, most likely due to compound-specific stress [15]. Only M. lenta strains R-45370 and R-45377 grew in the presence of 100 mM nitrate and tolerated higher concentrations of nitrate than ammonium (maximum of 40 mM), whilst also showing the highest salt tolerance regardless of their nitrogen source (200 mM NaCl). The other strains tolerated higher sodium chloride additions than equimolar nitrate additions, again suggesting concentration-dependent nitrate inhibition.

Assimilation and toxicity of the potential intermediates nitrite and hydroxylamine

Ammonium amendments introduce a fraction of ammonia to the culture depending on the pH (NH3/NH4 +; pKa = 9.23). Ammonia can be toxic to methanotrophs as it functions as a competitive inhibitor of MMO or leads to accumulation of hydroxylamine and nitrite, toxic products of its oxidation. Tolerance of methanotrophs to ammonia can thus be dependent of intrinsic toxicity levels of hydroxylamine and nitrite as well as their ability to use either of them for assimilation. This was again tested qualitatively in microtiter plates using growth as a proxy for methane oxidation.

For our strain panel, preliminary experiments showed that none of the strains could grow with 1 mM or 2 mM hydroxylamine as sole nitrogen source. Therefore, tolerance of hydroxylamine was tested by providing 2 mM ammonium for assimilation and spiking of 0.01 mM, 1 mM and 2 mM hydroxylamine. None of the strains could grow in the presence of 2 mM hydroxylamine. Eight strains exhibited growth when 0.01 mM and 1 mM hydroxylamine was added, while eight other strains did not even show growth at a concentration of only 0.01 mM hydroxylamine (Table 1).

All Methylomonas strains were able to grow with up to 2 mM nitrite as sole nitrogen source, demonstrating nitrite tolerance as well as assimilation. The type Ib strain R-49797 tolerated the highest nitrite concentration (up to 5 mM). However, this strain was sensitive to hydroxylamine, even at concentrations of 0.01 mM. Type II strain could not use nitrite as sole nitrogen source.

Production of nitrite and nitrous oxide from nitrate and ammonium

To evaluate nitrite and nitrous oxide production from nitrate or ammonium, strains were grown in batch cultures at an initially high oxygen tension (O2 levels in air). Because of methanotrophic activity, oxygen concentrations gradually decreased to levels too low to support further methane oxidation, thus inducing stationary growth phase. Most strains clearly produced nitrite (15 out of 16) and nitrous oxide (13 out of 16) from nitrate, while production of nitrous oxide, but not nitrite, from ammonium was also a general feature (14 out of 16 strains). Nitrite production from ammonium was only apparent for Methylosinus sp. R-45379 (Type II) but near detection limit (10 μM) for M. methanica R-45371 and M. lenta R-45370 and R-45377. The strain panel could be divided into eight different dissimilatory nitrogen phenotypes, based on detection of nitrite, nitrous oxide or both (Table 2); onset of N-species production or amount produced was not taken into account. An example of each phenotype is displayed in Figure 1. It should be noted that monitoring only started at late exponential phase (day 6), as preliminary experiments then showed the onset of nitrous oxide production. Therefore, influence of nitrate or ammonium on actual methane oxidation rate was not assessed, although small amounts of methane were still consumed (Additional file 6: Figure S2) and final methane concentration consumed with either N source did not differ per strain.

Table 2 Production of nitrite and nitrous oxide from nitrate or ammonium per strain (n = 2)
Full size table
Figure 1
figure1

Specific nitrite and nitrous oxide production profiles for assigned phenotypes. Nitrite (circles) and nitrous oxide (squares) production of methanotrophic strains cultivated in nitrate medium (dNMS, solid line) and ammonium medium (dAMS, dashed line). Nitrous oxide values showed are for total vial and were corrected to N2O-N to allow equimolar nitrogen comparison with NO2 −. The Y-axis could not be made uniform for all strains for clarity; care should be taken when interpreting the data between strains. Phenotype I is represented by M. methanica NCIMB 11130T, phenotype II by M. koyamae R-45378, phenotype III by M. methanica R-45363, phenotype IV by M. methanica R-45371, phenotype V by M. koyamae R-45383, phenotype VI by M. koyamae R-49807, phenotype VII by M. lenta R-45370, Phenotype VIII by Methylosinus sp. R-45379.

Full size image

Detectable amounts of nitrite were produced from nitrate, used as sole nitrogen source, in all strains once oxygen concentrations became low. The only exception was M. methanica R-45363 (Table 2; Figure 1: phenotype III). When growth and methane oxidation activity ceased due to oxygen limitation, no additional nitrite was produced, but several strains (Figure 1: phenotype II and VI) showed a slow decrease in nitrite levels with a corresponding rise in nitrous oxide over time (Table 2). This was most clear for M. koyamae R-49807, as for this strain from the start of the incubation at high oxygen tension (O2 levels in air) until day six (approximately 1.7% v/v O2), methane was oxidized but no nitrite or nitrous oxide could be measured. At day nine, nitrite levels of approximately 400 μM were measured at oxygen levels below 0.3% v/v, and from that point onwards, until the end of the incubation at day 21, nitrite levels dropped with a corresponding rise in nitrous oxide levels, while no more methane oxidation occurred. M. koyamae R-45383 produced nitrite but did not produce nitrous oxide (Table 2; Figure 1: phenotype V). M. methanica NCIMB 11130T and R-45364 and Methylosinus sp. R-45379 produced both nitrite and nitrous oxide, but did not show a subsequent drop in nitrite and corresponding rise in nitrous oxide (Table 2; Figure 1: phenotypes I, IV and VIII). M. methanica R-45371 produced nitrous oxide and small amounts of nitrite, approximating the detection limit of the assay (10 μM).

With ammonium as sole nitrogen source, M. methanica R-45371, M. lenta R-45370 and R-45377, and Methylosinus sp. R-45379 (Table 2; Figure 1: phenotypes IV, VII and VIII respectively) produced both measurable levels of nitrite and nitrous oxide. Interestingly, between day six and nine, a fraction of the produced nitrite seems to be converted into nitrous oxide, after which both nitrite and nitrous oxide levels remained stable over time [Table 2; Figure 1: phenotypes IV and VIII (phenotype VII deviates because of slow growth)]. Most strains were able to produce nitrous oxide without preceding measureable levels of nitrite.

Discussion

The ability of Methylomonas strains to produce nitrite and nitrous oxide from moderate levels (10 mM) of nitrate and ammonium, indicative of detoxification, demonstrated metabolic variability on both genus- and species level (Table 2; Figure 1). Ammonium amendments introduce a fraction of ammonia to the culture depending on the pH, which can be oxidized to hydroxylamine by methane monooxygenase. The conversion of hydroxylamine directly to nitric oxide or indirectly via nitrite is well studied and limited to the activity of hydroxylamine oxidoreductase [8–10], and to a much lesser extent cytochrome P460 [6]. In contrast, nitrate metabolism is underexplored in methanotrophs and little is known, except that nitrite from nitrate can be produced by both assimilatory and dissimilatory nitrate reductases [6, 28]. Nevertheless, high levels of nitrite produced from nitrate should also be converted to nitric oxide for nitrite detoxification. Upon production, the cytotoxic nitric oxide needs to be immediately detoxified to the, at least for the cell, harmless nitrous oxide by one of the many known nitric oxide reductase enzymes [29–33]. In the present study, most strains were able to produce nitrous oxide from ammonium without preceding measurable levels of nitrite, either due to an immediate conversion of hydroxylamine to nitric oxide by hydroxylamine oxidoreductase or to small transient nitrite peaks below detection levels. The latter hypothesis is plausible when considering the nearly identical nitrous oxide profiles observed for M. methanica NCIMB 11130T and Methylosinus sp. R-45379, except the nitrite peak (Figure 1: phenotypes I and VIII), suggesting the same detoxification mechanism. Nitrate as sole nitrogen source was converted to nitrite in all strains once oxygen concentrations became low, except for M. methanica R-45363 that probably lacks an enzyme for nitrate reduction. Strains of both M. methanica and M. koyamae showed a drop in nitrite levels with a corresponding rise in nitrous oxide levels (Table 2; Figure 1). These observations would fit nicely with activities of an oxygen-sensitive nitrate reductase producing nitrite in actively growing cells, which is subsequently detoxified to nitrous oxide (via nitric oxide, not measured in this study) during stationary phase, similar to previous observations for non-denitrifiers [34, 35], but unreported in methanotrophs. M. methanica NCIMB 11130T and R-45364 produced both nitrite and nitrous oxide from nitrate, but did not show a subsequent drop in nitrite and corresponding rise in nitrous oxide (Table 2; Figure 1: phenotypes I, IV and VIII). M. koyamae R-45383 was the only strain not able to produce nitrous oxide from either nitrate or ammonium, probably because it lacks a nitric oxide reductase. On the other hand, M. koyamae strain R-49807 did produce nitrous oxide from nitrate but not from ammonium. This indicates that the nitrous oxide produced was truly derived directly from nitrate via nitrite, and not via an indirect process via ammonium, i.e. assimilatory reduction of nitrate to ammonium. It is clear that, although variable phenotypes for nitrite and nitrous oxide production from nitrate and ammonium can be tentatively explained using the currently described genomic inventories of other methanotrophs [6] or a combination thereof, various novel features on specifically nitrate reduction should be the subject of further genome and expression studies.

Within a single species, strain-dependent differences were also observed. This was most obvious for strains within M. koyamae regarding their tolerance to high ammonium levels. Noteworthy are the identical 16S rRNA gene and (almost) identical functional gene sequences between the highly ammonium-tolerant M. koyamae strains NCIMB 14606T and R-49799 (up to 100 mM) and the low ammonium-tolerant strain R-49807 (up to 40 mM) (Additional file 2: Figure S4 and Additional file 4: Figure S5; Additional file 3: Table S1 and Additional file 5: Table S2). This differentiation among M. koyamae strains is further demonstrated in their tolerance to hydroxylamine (up to 1 mM). In addition, R-49807 unexpectedly did not exhibit N2 fixation, as sole M. koyamae strain, despite a >99% nifH gene sequence similarity with strains NCIMB 14606T and R-49799, both positive for N2 fixation under low oxygen tension. This might be explained by a higher oxygen sensitivity of the nitrogenase of this strain [14, 36], requiring oxygen concentrations lower than the 2% used here. In addition, something worth considering as well is the applicability of M. koyamae R-49799 for methane mitigation in high-ammonium sites, since this strain grows at 100 mM ammonium levels, utilizes 2 mM nitrite as sole nitrogen source, tolerates hydroxylamine levels up to 1 mM and possesses pathways to detoxify ammonia and nitrite.

Some features appeared to be general within Methylomonas with some strain specific exceptions. The observed higher tolerance to ammonium than nitrate confirmed previous reports of methanotrophic growth inhibition above 40 mM nitrate [37, 38]. Nevertheless, two M. lenta strains (R-45370 and R-45377) tolerated nitrate concentrations up to 100 mM. This could not be linked to a possible higher nitrite tolerance, as all strains could grow with up to 2 mM nitrite as sole nitrogen source. This nitrite tolerance and assimilation was in contrast to earlier findings that nitrite utilization was rare for M. methanica members [7]. The presence of the nifH gene and the ability to fix nitrogen with an oxygen-sensitive nitrogenase was also found in most strains, although both traits appear to be strain-dependent when combining the results of this study with other reports [12]. Although initially thought to be limited to mostly Type II and Type Ib methanotrophs [11], our findings are in agreement with more recent reports suggesting that nitrogen fixation is a common feature of many methanotrophs, including Type Ia and verrucomicrobial methanotrophs [12–14].

Conclusions

Microbial ecologists still struggle to link microbial community structure to ecosystem functioning, notwithstanding that in-depth analyses of microbial community structure has never been easier than now, with the affordability of deep sequencing of amplified genes as well as whole communities. But to make sense out of sequence data, basic knowledge about the biology of the microorganisms involved in the biogeochemical functions under study is pivotal. Unfortunately, current insights are often retrieved from sporadic pure culture studies including only few distantly related strains. Here, investigation of closely related, genotypically different methanotrophic strains revealed differential responses to overcome inhibition and toxicity from high nitrogen loads and assimilation of various nitrogen sources, yielding competitive fitness advantages to individual methane-oxidizing bacteria. We have not assessed the specific effect of nitrogen on methanotrophic activity rate, but rather demonstrated the surprising versatility below the commonly used cut-off for operational taxonomic units, i.e. genus level. Our results proved that community structure at the deepest phylogenetic resolution potentially influences in situ functioning. Until molecular tools become available to allow much finer analyses of microbial diversity, metabolic variability at those unmeasurable levels should be taken into account.

Methods

Bacterial strains and standard growth conditions

Fourteen of the sixteen tested strains were members of the genus Methylomonas: the type strain Methylomonas methanica NCIMB 11130T and six strains R-45362, R-45363, R-45364, R-45371, R-45372 and R-45374 most closely related to this type strain (98.3-98.6% 16S rRNA sequence similarity; further referred to as M. methanica strains); the type strain Methylomonas koyamae NCIMB 14606T and four strains R-45378, R-45383, R-49799 and R-49807 most closely related to this type strain (97.9-100% 16S rRNA sequence similarity; further referred to as M. koyamae strains); two strains Methylomonas sp. R-45370 and R-45377 most closely related to the no-longer extant type strain of M. scandinavica (97.5% 16S rRNA sequence similarity) and recently described as novel species Methylomonas lenta[39]. All Methylomonas strains were genetically different as determined by GTG5 rep-PCR fingerprinting [40]. In addition, two non-Methylomonas strains were included as a reference: Methylococcaceae sp. R-49797, a member of the Methylococcus-Methylocaldum-Methylogaea clade (Type Ib) and Methylosinus sp. R-45379 (Type II). Included strains were obtained from various origins: strains R-45362, R-45363, R-45364, R-45371, R-45372, R-45374 and R-45370 were isolated from the top layer of a denitrification tank of a waste water treatment plant, strain R-45377 was isolated from a slurry pit of a cow stable; strains R-45378, R-45383 and R-45379 were isolated from a wetland [40]; strains R-49807 and R-49797 were isolated from a facultative waste stabilization pond in South Africa. Strain R-49799 was isolated from a high ammonium (70 mM) methanotrophic enrichment from a mixture of inocula (compost heap, top soil with leaf litter, anaerobic sludge and a wastewater treatment plant). All strains were routinely subcultured on diluted nitrate mineral salts (dNMS) plates [41] and incubated in gastight jars (Oxoid, UK) under a CH4 : air (1 : 1) atmosphere. The composition of dNMS in this study was the following: 2 mM KNO3, 4 mM MgSO4, 0.9 mM CaCl2, 2 mM Na2HPO4/KH2PO4 buffer (pH 6.8), 14 μM ferric-sodium-EDTA and a trace element solution [25] with Cu2+ concentration adjusted to 10 μM. Fresh colonies from one-week grown cultures on dNMS plates were used as start inoculum (OD600nm 0.01, final concentration) for the different growth experiments performed in this study. To be able to reach comparable cell densities, two-week grown cultures were used for the two slower-growing strains M. lenta R-45370 and R-45377.

Assessment of nitrogen assimilation and toxicity

The ability of the strains to grow in the presence of a range of concentrations of NaNO3, KNO3, NH4Cl and (NH4)2SO4-N (2, 10, 20, 40, 150 and 200 mM) and NaNO2 (2, 5, 10 mM) was assessed. In order to evaluate general osmotic influences, sodium chloride tolerance was also tested in dNMS and dAMS (identical medium composition with ammonium instead of nitrate as sole nitrogen source), each supplemented with 40, 100, 150 and 200 mM NaCl. Hydroxylamine tolerance was evaluated in dAMS supplemented with 0.01, 1 and 2% (w/v) hydroxylamine. Initial cultivation experiments showed that strains cultivated with ammonium consistently preferred a 10 mM buffer over a 2 mM buffer, while the opposite was observed with nitrate as nitrogen source. Therefore, in this study, dNMS (nitrate, nitrite or nitrogen-free medium, see below) media contained a 2 mM phosphate buffer, while dAMS (ammonium) media contained a 10 mM phosphate buffer. Besides nitrogen source and buffer concentration, all other components were identical between media.

All strains were inoculated in duplicate in liquid media in sterile 96-well microtiter plates (300 μL, final volume per well). Cultures were incubated under a CH4 : air (1 : 1) atmosphere at optimal temperature (20°C for strains R-45370, R-45371 and R-45377 and 28°C for the other strains). Growth was monitored and verified by visual inspection after 4, 7, 11, 14 and 21 days of incubation.

Assessment of production of nitrite and nitrous oxide

Initial experiments on a limited number of Methylomonas strains showed that nitrous oxide was produced in cultures grown with ammonium or nitrate as sole nitrogen source once a stationary phase was induced via oxygen depletion, while nitrogen was not depleted. Nitrous oxide production was never detected in nitrite-containing media that were not inoculated or in cultures with nitrite levels too high to support growth and activity, ruling out nitrous oxide production from nitrite from a non-biological origin. Therefore, all strains were cultivated in dAMS with 10 mM NH4Cl and in dNMS with 10 mM KNO3 (a high enough nitrogen concentration to prevent nitrogen depletion in our batch setup) in gastight serum vials under a 20% CH4 in air atmosphere and time points were selected to include only the stationary phase (expected to start before or around day six, except for several slower growing cultures such as Methylomonas lenta R-45370 and R-45377), namely after 6, 9, 14 and 21 days of incubation. Growth, methane oxidation activity, either nitrate or ammonium consumption, and nitrite and nitrous oxide production were assessed. In this batch setup, oxygen was the growth-limiting factor, and thus the setup does not allow to distinguish between effects caused by cells entering the stationary phase or by oxygen limitation.

Analytical methods

Methane oxidation activity was assessed by monitoring of CH4, O2 and CO2 levels via gas chromatography using a Compact GC (Global Analyzer Solutions, Belgium) equipped with two columns (O2/N2 and CO2/N2O separation) connected to a thermal conductivity detector and one column (CH4 levels) connected to a flame ionization detector. The change in gas pressure due to methane oxidation was monitored with an Infield 7 pressure meter (UMS, Germany). Values measured by gas chromatography were converted to μmol gas Lliquid −1 by compensating for change in gas pressure and taking the solubility of the gases into account. Colorimetric assays were performed to determine the nitrite [42], nitrate [43] and ammonium [44] concentration. Growth was monitored via OD600nm and, when necessary, converted to mg protein via the correlation factor 243.77 obtained from previous growth experiments [45] (Additional file 7: Figure S3). For miniaturized screening set up, growth was scored positive when the average OD600nm value became larger than the average initial OD600nm value added by 5-times its standard deviation. Growth correlated very well with methane oxidation (Additional file 1: Figure S1) and was therefore used as a proxy thereof.

Nitrogen fixation

Strains were inoculated in duplicate as explained above in liquid nitrogen-free dNMS in gastight flasks under a 20% CH4 in air atmosphere (approximately 21% O2, high oxygen tension condition) and under a 20% CH4 in ten-fold diluted air (with helium) atmosphere (approximately 2.1% O2, low oxygen tension condition). In addition to the Type Ib strain for which nifH gene amplification was negative, four extra methanotrophic strains without the nifH gene were included as negative controls, which indeed all did not demonstrate growth because of inability to fix dinitrogen. Growth was determined through OD600nm measurements and verified by visual inspection after 4, 7, 11, 14 and 21 days of incubation. In addition, the methane oxidation activity was assessed by gas chromatography. Absence of nitrate (below 0.15 mM), ammonium (below 0.15 mM) and nitrite (below 10 μM) in nitrogen-free dNMS was confirmed via colorimetry.

pmoA and nifHgene sequence analyses

DNA was extracted by alkaline lysis [46]. Amplification of pmoA gene encoding the particulate methane monooxygenase, the key enzyme for methane oxidation, was performed using the primer set A189f/mb661r as described previously [47]. Amplification of the nifH gene encoding the highly conserved Fe protein of nitrogenase was performed using the primer set F1/nifH439R, the PCR mix and temperature program as described by De Meyer et al. [48]. When amplification was positive, gene sequences were generated and sequences were assembled with the BioNumerics 5.1 software (Applied Maths, Belgium). Protein translation analysis using Transeq (http://www.ebi.ac.uk/tools/emboss/transeq) and pBLAST [49] confirmed the genes encoding functions.

Nucleotide sequence accession numbers

The nifH gene sequence data generated in this study have been deposited in GenBank/EMBL/DDBJ with accession numbers HF954360, HF954362 and HF954366 to HF954376. The pmoA gene sequence data generated in this study have been deposited in GenBank/EMBL/DDBJ with accession numbers HF954359, HF954361, HF954363 and from HG915717 to HG915727.

References

  1. 1.

    Denman KL, Brasseur G, Chidthaisong A, Ciais P, Cox PM, Dickinson RE, Hauglustaine D, Heinze C, Holland E, Jacob D, Lohmann U, Ramachandran S, da Silva Dias PL, Wofsy SC, Zhang X: Couplings Between Changes in the Climate System and Biogeochemistry. Climate Change 2007: The Physical Science Basis Contribution of Working Group I to the Fourth Assessment Report of the Intergovernmental Panel on Climate Change. Edited by: Solomon S, Qin D, Manning M, Chen Z, Marquis M, Averyt KB, Tignor M, Miller HL. 2007, Cambridge, United Kingdom and New York, NY, USA: Cambridge University Press

  2. 2.

    Semrau JD, DiSpirito AA, Yoon S: Methanotrophs and copper. FEMS Microbiol Rev. 2010, 34: 496-531.

  3. 3.

    Dedysh SN: Exploring methanotroph diversity in acidic northern wetlands: Molecular and cultivation-based studies. Microbiology. 2009, 78: 655-669. 10.1134/S0026261709060010.

  4. 4.

    Hanson RS, Hanson TE: Methanotrophic bacteria. Microbiol Rev. 1996, 60: 439-471.

  5. 5.

    Op den Camp HJM, Islam T, Stott MB, Harhangi HR, Hynes A, Schouten S, Jetten MSM, Birkeland NK, Pol A, Dunfield PF: Environmental, genomic and taxonomic perspectives on methanotrophic Verrucomicrobia. Environ Microbiol Rep. 2009, 1: 293-306. 10.1111/j.1758-2229.2009.00022.x.

  6. 6.

    Stein LY, Klotz MG: Nitrifying and denitrifying pathways of methanotrophic bacteria. Biochem Soc Trans. 2011, 39: 1826-1831. 10.1042/BST20110712.

  7. 7.

    Bowman JP, Sly LI, Nichols PD, Hayward AC: Revised taxonomy of the methanotrophs - Description of Methylobacter Gen-Nov, emendation of Methylococcus, validation of Methylosinus and Methylocystis species, and a proposal that the family Methylococcaceae includes only the group-I methanotrophs. Int J Syst Bacteriol. 1993, 43: 735-753. 10.1099/00207713-43-4-735.

  8. 8.

    Nyerges G, Han SK, Stein LY: Effects of Ammonium and Nitrite on Growth and Competitive Fitness of Cultivated Methanotrophic Bacteria. Appl Environ Microbiol. 2010, 76: 5648-5651. 10.1128/AEM.00747-10.

  9. 9.

    Campbell MA, Nyerges G, Kozlowski JA, Poret-Peterson AT, Stein LY, Klotz MG: Model of the molecular basis for hydroxylamine oxidation and nitrous oxide production in methanotrophic bacteria. FEMS Microbiol Lett. 2011, 322: 82-89. 10.1111/j.1574-6968.2011.02340.x.

  10. 10.

    Nyerges G, Stein LY: Ammonia cometabolism and product inhibition vary considerably among species of methanotrophic bacteria. FEMS Microbiol Lett. 2009, 297: 131-136. 10.1111/j.1574-6968.2009.01674.x.

  11. 11.

    Murrell JC, Dalton H: Nitrogen-fixation in obligate methanotrophs. J Gen Microbiol. 1983, 129: 3481-3486.

  12. 12.

    Auman AJ, Speake CC, Lidstrom ME: nifH sequences and nitrogen fixation in type I and type II methanotrophs. Appl Environ Microbiol. 2001, 67: 4009-4016. 10.1128/AEM.67.9.4009-4016.2001.

  13. 13.

    Boulygina ES, Kuznetsov BB, Marusina AI, Turova TP, Kravchenko IK, Bykova SA, Kolganova TV, Gal'chenko VF: Study of nucleotide sequences of nifH genes in methanotrophic bacteria. Mikrobiologiia. 2002, 71: 500-508.

  14. 14.

    Khadem AF, Pol A, Jetten MS, Op den Camp HJ: Nitrogen fixation by the verrucomicrobial methanotroph ‘Methylacidiphilum fumariolicum’ SolV. Microbiology. 2010, 156: 1052-1059. 10.1099/mic.0.036061-0.

  15. 15.

    King GM, Schnell S: Effects of ammonium and non-ammonium salt additions on methane oxidation by Methylosinus trichosporium OB3b and Maine forest soils. Appl Environ Microbiol. 1998, 64: 253-257.

  16. 16.

    Schnell S, King GM: Mechanistic analysis of ammonium inhibition of atmospheric methane consumption in forest soils. Appl Environ Microbiol. 1994, 60: 3514-3521.

  17. 17.

    Bodelier PL, Roslev P, Henckel T, Frenzel P: Stimulation by ammonium-based fertilizers of methane oxidation in soil around rice roots. Nature. 2000, 403: 421-424. 10.1038/35000193.

  18. 18.

    Noll M, Frenzel P, Conrad R: Selective stimulation of type I methanotrophs in a rice paddy soil by urea fertilization revealed by RNA-based stable isotope probing. FEMS Microbiol Ecol. 2008, 65: 125-132. 10.1111/j.1574-6941.2008.00497.x.

  19. 19.

    Mohanty SR, Bodelier PLE, Floris V, Conrad R: Differential effects of nitrogenous fertilizers on methane-consuming microbes in rice field and forest soils. Appl Environ Microbiol. 2006, 72: 1346-1354. 10.1128/AEM.72.2.1346-1354.2006.

  20. 20.

    Bodelier PLE, Laanbroek HJ: Nitrogen as a regulatory factor of methane oxidation in soils and sediments. FEMS Microbiol Ecol. 2004, 47: 265-277. 10.1016/S0168-6496(03)00304-0.

  21. 21.

    Ho A, Kerckhof F-M, Luke C, Reim A, Krause S, Boon N, Bodelier PL: Conceptualizing functional traits and ecological characteristics of methane-oxidizing bacteria as life strategies. Environ Microbiol Rep. 2013, 5 (3): 335-345. 10.1111/j.1758-2229.2012.00370.x.

  22. 22.

    Vandamme P, Pot B, Gillis M, DeVos P, Kersters K, Swings J: Polyphasic taxonomy, a consensus approach to bacterial systematics. Microbiol Rev. 1996, 60: 407-438.

  23. 23.

    Johnson ZI, Zinser ER, Coe A, McNulty NP, Woodward EMS, Chisholm SW: Niche Partitioning Among Prochlorococcus Ecotypes Along Ocean-Scale Environmental Gradients. Science. 2006, 311: 1737-1740. 10.1126/science.1118052.

  24. 24.

    Hunt DE, David LA, Gevers D, Preheim SP, Alm EJ, Polz MF: Resource Partitioning and Sympatric Differentiation Among Closely Related Bacterioplankton. Science. 2008, 320: 1081-1085. 10.1126/science.1157890.

  25. 25.

    Bowman J: The Methanotrophs - The Families Methylococcaceae and Methylocystaceae. Chapter 3.1.14. The Prokaryotes, Volume 5. Edited by: Dworkin M, Falkow S, Rosenberg E, Schleifer K-H, Stackebrandt E. 2006, 266-289. Third

  26. 26.

    Ogiso T, Ueno C, Dianou D, Huy TV, Katayama A, Kimura M, Asakawa S: Methylomonas koyamae sp nov., a type I methane-oxidizing bacterium from floodwater of a rice paddy field. Int J Syst Evol Microbiol. 2012, 62: 1832-1837. 10.1099/ijs.0.035261-0.

  27. 27.

    Danilova OV, Kulichevskaya IS, Rozova ON, Detkova EN, Bodelier PL, Trotsenko YA, Dedysh SN: Methylomonas paludis sp. nov., the first acid-tolerant member of the genus Methylomonas, from an acidic wetland. Int J Syst Evol Microbiol. 2012, 63: 2282-2289.

  28. 28.

    Anthony C: Biochemistry of methylotrophs. 1982, London: The Academic Press

  29. 29.

    Vine CE, Cole JA: Nitrosative stress in Escherichia coli: reduction of nitric oxide. Biochem Soc Trans. 2011, 39: 313-315.

  30. 30.

    Zumft WG: Nitric oxide reductases of prokaryotes with emphasis on the respiratory, heme–copper oxidase type. J Inorg Biochem. 2005, 99: 194-215. 10.1016/j.jinorgbio.2004.09.024.

  31. 31.

    Zumft WG, Braun C, Cuypers H: Nitric oxide reductase from Pseudomonas stutzeri. Primary structure and gene organization of a novel bacterial cytochrome bc complex. Eur J Biochem. 1994, 219: 418-490.

  32. 32.

    Hino T, Nagano S, Sugimoto H, Tosha T, Shiro Y: Molecular structure and function of bacterial nitric oxide reductase. Biochim Biophys Acta. 1817, 2011: 680-687.

  33. 33.

    Stein LY: Surveying N2O-producing pathways in bacteria. Methods in Enzymology: research on nitrification and related processes, Volume 486. Edited by: Klotz MG. 2011, San Diego: Elsevier Academic Press, 131-152.

  34. 34.

    Smith MS, Zimmerman K: Nitrous oxide production by nondenitrifying soil nitrate reducers. Soil Sci Soc Am J. 1981, 45: 865-871. 10.2136/sssaj1981.03615995004500050008x.

  35. 35.

    Smith MS: Nitrous oxide production by Escherichia coli is correlated with nitrate reductase activity. Appl Environ Microbiol. 1983, 45: 1545-1547.

  36. 36.

    Vorob'ev AV, Dedysh SN: Inadequacy of enrichment culture technique for assessing the structure of methanotrophic communities in peat soil. Microbiology. 2008, 77: 504-507. 10.1134/S0026261708040188.

  37. 37.

    Park SH, Shah NN, Taylor RT, Droege MW: Batch cultivation of Methylosinus trichosporium OB3b. 2. Production of particulate methane monooxygenase. Biotechnol Bioeng. 1992, 40: 151-157. 10.1002/bit.260400121.

  38. 38.

    Lee SW, Im J, DiSpirito AA, Bodrossy L, Barcelona MJ, Semrau JD: Effect of nutrient and selective inhibitor amendments on methane oxidation, nitrous oxide production, and key gene presence and expression in landfill cover soils: characterization of the role of methanotrophs, nitrifiers, and denitrifiers. Appl Microbiol Biotechnol. 2009, 85: 389-403. 10.1007/s00253-009-2238-7.

  39. 39.

    Hoefman S, Heylen K, de Vos P: Methylomonas lenta sp. nov., a methanotroph isolated from manure and a denitrification tank in Belgium. Int J Syst Evol Microbiol. 2014, 4: doi: 10.1099/ijs.0.057794-0

  40. 40.

    Hoefman S, van der Ha D, De Vos P, Boon N, Heylen K: Miniaturized extinction culturing is the preferred strategy for rapid isolation of fast-growing methane-oxidizing bacteria. Microb Biotechnol. 2012, 5: 368-378. 10.1111/j.1751-7915.2011.00314.x.

  41. 41.

    Dunfield PF, Khmelenina VN, Suzina NE, Trotsenko YA, Dedysh SN: Methylocella silvestris sp nov., a novel methanotroph isolated from an acidic forest cambisol. Int J Syst Evol Microbiol. 2003, 53: 1231-1239. 10.1099/ijs.0.02481-0.

  42. 42.

    Griess P: Bemerkungen zu der abhandlung der H.H. Weselsky und Benedikt “Ueber einige azoverbindungen”. Chem Ber. 1879, 12: 426-428. 10.1002/cber.187901201117.

  43. 43.

    Cataldo DA, Maroon M, Schrader LE, Youngs VL: Rapid colorimetric determination of nitrate in plant tissue by nitration of salicylic acid. Commun Soil Sci Plant Anal. 1975, 6: 71-80. 10.1080/00103627509366547.

  44. 44.

    Taylor S, Ninjoor V, Dowd DM, Tappel AL: Cathepsin B2 measurement by sensitive fluorometric ammonia analysis. Anal Biochem. 1974, 60: 153-162. 10.1016/0003-2697(74)90140-7.

  45. 45.

    Hoefman S, van der Ha D, Boon N, Vandamme P, De Vos P, Heylen K: Customized media based on miniaturized screening improve growth rate and cell yield of methane-oxidizing bacteria of the genus Methylomonas. Antonie Van Leeuwenhoek. 2014, 105: 353-366. 10.1007/s10482-013-0083-2.

  46. 46.

    Coenye T, Spilker T, Martin A, LiPuma JJ: Comparative assessment of genotyping methods for epidemiologic study of Burkholderia cepacia genomovar III. J Clin Microbiol. 2002, 40: 3300-3307. 10.1128/JCM.40.9.3300-3307.2002.

  47. 47.

    Costello AM, Lidstrom ME: Molecular Characterization of Functional and Phylogenetic Genes from Natural Populations of Methanotrophs in Lake Sediments. Appl Environ Microbiol. 1999, 65: 5066-5074.

  48. 48.

    De Meyer SE, van Hoorde K, Vekeman B, Braeckman T, Willems A: Genetic diversity of rhizobia associated with indigenous legumes in different regions of Flanders (Belgium). Soil Biol Biochem. 2011, 43: 2384-2396. 10.1016/j.soilbio.2011.08.005.

  49. 49.

    Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ: Basic local alignment search tool. J Mol Biol. 1990, 215: 403-410.

  50. 50.

    Ludwig W, Strunk O, Westram R, Richter L, Meier H, Yadhukumar , Buchner A, Lai T, Steppi S, Jobb G, Förster W, Brettske I, Gerber S, Ginhart AW, Gross O, Grumann S, Hermann S, Jost R, König A, Liss T, Lüssmann R, May M, Nonhoff B, Reichel B, Strehlow R, Stamatakis A, Stuckmann N, Vilbig A, Lenke M, Ludwig T, Bode A, Schleifer KH: ARB: a software environment for sequence data. Nucleic Acids Res. 2004, 32: 1363-1371. 10.1093/nar/gkh293.

  51. 51.

    Tamura K, Peterson D, Peterson N, Stecher G, Nei M, Kumar S: MEGA5: molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods. Mol Biol Evol. 2011, 28: 2731-2739. 10.1093/molbev/msr121.

Download references

Acknowledgements

This work was funded by the Geconcerteerde Onderzoeksactie (GOA) of Ghent University (BOF09/GOA/005). Kim Heylen is supported by the Flemish Fund for Scientific Research (FWO11/PDO/084). David van der Ha is supported by the Institute for the Promotion of Innovation through Science and Technology in Flanders (IWT-Vlaanderen, SB-83259). The authors greatly acknowledge Lisa Stein and K. Dimitri Kits for critically reading an earlier version of the manuscript.

Author information

Affiliations

  1. Laboratory of Microbiology, Department of Biochemistry and Microbiology, Ghent University, Ghent, Belgium

    • Sven Hoefman
    • , Peter Vandamme
    • , Paul De Vos
    •  & Kim Heylen

  2. Laboratory of Microbial Ecology and Technology (LabMET), Ghent University, Coupure Links 653, B-9000, Ghent, Belgium

    • David van der Ha
    •  & Nico Boon

  3. BCCM/LMG Bacteria Collection, Ghent, Belgium

    • Paul De Vos

Authors

  1. Search for Sven Hoefman in:

  2. Search for David van der Ha in:

  3. Search for Nico Boon in:

  4. Search for Peter Vandamme in:

  5. Search for Paul De Vos in:

  6. Search for Kim Heylen in:

Corresponding author

Correspondence to Kim Heylen.

Additional information

Competing interests

The authors declare to have no competing interests.

Authors’ contributions

SH and KH conceived and designed experiment, interpreted data and wrote the manuscript. SH acquired and analysed data. DvdH, NB, PV and PdV critically revised the manuscript. All authors read and approved the final manuscript.

Electronic supplementary material

Additional file 1: Figure S1: Correlation between growth (OD600nm) and methane consumption. In general, growth correlates well with methane oxidation (A), validating the use of growth as a proxy for methane oxidation (n = 8). However, the correlation between growth and methane oxidation is influenced by growth rate and growth medium. When taken this into account for a single strain, both parameters correlate even better, as exemplified for R-45374 in dNMS (B). (TIFF 4 MB)

Additional file 2: Figure S4: 16S rRNA gene phylogenetic neighbor-joining tree. The publically available 16S rRNA gene sequences of the strains included in this study were aligned with type strains of the remaining species of the genus Methylomonas using the integrated aligner of ARB [50]. Based on the 16S rRNA gene alignment, a neighbor joining tree was constructed using the MEGA 5 software [50]. The maximum composite likelihood method was used and 1186 positions were taken into account. Bootstrap analysis based on 500 replicates was performed. Bootstrap values below 70% are not shown. Bar: 0.02 substitutions per nucleotide position. (TIFF 7 MB)

Additional file 3: Table S1: Estimates of Evolutionary Divergence between 16S rRNA gene sequences. The number of base substitutions per site between 16S rRNA gene sequences are shown. Pairwise distance analyses were conducted based on the alignment used in Additional file 4: Figure S4. Evolutionary analyses were conducted in MEGA5 [51]. (PDF 4 KB)

Additional file 4: Figure S5: pmoA gene phylogenetic neighbor-joining tree. The pmoA gene sequences of the strains included in this study and available pmoA gene sequences of type strains of the remaining species of the genus Methylomonas were aligned based on translated protein sequences and DNA-based neighbor joining trees constructed using MEGA5 [51]. The maximum composite likelihood method was used and 396 positions were taken into account. Bootstrap analysis based on 500 replicates was performed. Bootstrap values below 70% are not shown. Bar: 0.05 substitutions per nucleotide position. (PDF 11 KB)

Additional file 5: Table S2: Estimates of Evolutionary Divergence between pmoA gene sequences. The number of base substitutions per site between pmoA gene sequences are shown. Pairwise distance analyses were conducted based on the alignment used in Additional file 4: Figure S5. Evolutionary analyses were conducted in MEGA5 [51]. (PDF 4 KB)

Additional file 6: Figure S2: Methane consumption in late exponential to stationary phase in dNMS (A) or dAMS (B) per strain (n = 2). Assigned phenotypes are indicated between brackets. Error bars are high for R-45370 because of slow growth of one replicate. (TIFF 3 MB)

Additional file 7: Figure S3: Correlation between growth (OD600nm) and protein content. Data was taken from [45]. A correlation factor was extracted for conversion of growth to protein content. (TIFF 2 MB)

Authors’ original submitted files for images

Below are the links to the authors’ original submitted files for images.

Authors’ original file for figure 1

Rights and permissions

Reprints and Permissions

About this article

Keywords

  • Methylomonas methanica
  • Methylomonas koyamae
  • Methylomonas lenta
  • Strain dependency
  • Nitrogen assimilation
  • Detoxification

BMC Microbiology

ISSN: 1471-2180

Contact us