Skip to main content

Genome Scale Metabolic Model of the versatile methanotroph Methylocella silvestris



Methylocella silvestris is a facultative aerobic methanotrophic bacterium which uses not only methane, but also other alkanes such as ethane and propane, as carbon and energy sources. Its high metabolic versatility, together with the availability of tools for its genetic engineering, make it a very promising platform for metabolic engineering and industrial biotechnology using natural gas as substrate.


The first Genome Scale Metabolic Model for M. silvestris is presented. The model has been used to predict the ability of M. silvestris to grow on 12 different substrates, the growth phenotype of two deletion mutants (ΔICL and ΔMS), and biomass yield on methane and ethanol. The model, together with phenotypic characterization of the deletion mutants, revealed that M. silvestris uses the glyoxylate shuttle for the assimilation of C1 and C2 substrates, which is unique in contrast to published reports of other methanotrophs. Two alternative pathways for propane metabolism have been identified and validated experimentally using enzyme activity tests and constructing a deletion mutant (Δ1641), which enabled the identification of acetol as one of the intermediates of propane assimilation via 2-propanol. The model was also used to integrate proteomic data and to identify key enzymes responsible for the adaptation of M. silvestris to different substrates.


The model has been used to elucidate key metabolic features of M. silvestris, such as its use of the glyoxylate shuttle for the assimilation of one and two carbon compounds and the existence of two parallel metabolic pathways for propane assimilation. This model, together with the fact that tools for its genetic engineering already exist, paves the way for the use of M. silvestris as a platform for metabolic engineering and industrial exploitation of methanotrophs.


Methane is currently being released into the atmosphere at a rate over 70 million tonnes per year [1]. Given its high green-house potential, which, in a 20 year horizon, has been estimated to be 80 times that of CO2 [2], methane emissions constitute a serious environmental concern. Most of the methane emitted into the atmosphere is of biological origin, produced by methanogens in environments such as wetlands, although a substantial amount, 30% [3], occurs as natural gas arising from both anthropogenic and natural sources. This natural gas typically contains other short chain alkanes, principally ethane and propane, in addition to methane. The use of technologies such as fracking is expected to increase the importance of operational releases of natural gas [4]. The localized nature of many of these anthropogenic emissions, makes it possible to implement end-of-pipe abatement technologies. In this context, the use of methanotrophic organisms constitutes an efficient solution for methane abatement, and also offers the possibility of transforming a waste gas into marketable chemicals and commodities [5], thus contributing to the development of a circular economy. The cost of glucose, which is the most commonly used substrate in industrial biotechnology, can account for 30% of the total production costs, which makes methane a very attractive alternative [6].

The use of methanotrophs as platforms for metabolic engineering, requires both the development of techniques for their genetic manipulation and Genome Scale Metabolic Models (GSMMs) to design metabolic engineering strategies. Here we present the first GSMM of Methylocella silvestris. This is a versatile methanotroph that grows not only on methane but also on organic acids, alcohols [7] and short chain alkanes such as ethane and propane [8]. Bacteria of the genus Methylocella are abundant in many environments, including natural gas seeps [9, 10] and were also found among the microbial community following the Deepwater Horizon incident [11]. This may be linked to their ability to use ethane and propane as carbon sources and suggests that Methylocella could be a suitable platform for using natural gas as carbon source in industrial biotechnology, especially as genetic engineering tools have already been developed for this microorganism [12].

Currently, GSMMs have been published for 2 type I (gamma proteobacteria) methanotrophs, namely Methylomicrobium buryatense [13] and Methylomicrobium alcaliphilum [14], and 4 type II (alpha proteobacteria) methanotrophs of the genus Methylocystis [15, 16]. Methylocella silvestris is a type II methanotroph that uses the serine cycle for carbon assimilation, but differs from Methylocystis species in having a soluble methane monooxygenase (sMMO) [17] and a propane monooxygenase (PrMO) [8], while the Methylocystis species have only a membrane-associated particulate methane monooxygenase (pMMO) [18]. The metabolic implications of these differences are discussed later.

Previous work [8] showed that Methylocella silvestris oxidizes propane to a mixture of 1-propanol and 2-propanol. Most of the 2-propanol is produced by the soluble methane monooxygenase (sMMO), encoded by the genes Msil_1262–1267, while 1-propanol is mostly produced by a propane monooxygenase (PrMO), encoded by the genes Msil_1651–1648. This was proved by deleting the genes Msil_1262 and Msil_1651, encoding the alpha sub-units of each monooxygenase [8]. Other methanotrophs, such as Methylococcus capsulatus, have sMMO enzymes that can oxidize a broad range of alkanes and alkenes [19], however this organism lacks metabolic pathways to assimilate the resulting oxygenated intermediates. Methylocella silvestris is able to metabolize the oxidation products of ethane (ethanol and acetate) and, more interestingly, is able to metabolize both 1-propanol and 2-propanol via 2 different pathways which until now have not been fully elucidated.

The GSMM presented here enables the investigation of the distinct features of the metabolism of Methylocella in a systematic way, and the exploration of its potential as a platform for metabolic engineering. The model has been validated by testing its ability to predict growth (or absence of growth) on 12 different carbon sources, by comparing predicted and experimental biomass yields on methane and ethanol as well as by predicting the outcome of 2 different gene deletions. We also show how the model can be used as a scaffold for the analysis of proteomic data and serves to identify the enzymes whose change in abundance regulates the shift between different metabolic states and adaptation to different carbon sources.

Results and discussion

Metabolic model of Methylocella silvestris

A GSMM of Methylocella silvestris BL2 was constructed by annotating its genome [Joint Genome Institute (JGI) DSM 15510] using RAST [20] and obtaining an initial draft model with SEED [21]. The draft model was curated as described in Materials and methods. Specific pathways such as those involved in the degradation of propane, have been introduced based both in the genomic annotation and experimental evidence from enzymatic tests and mutants generated by gene knockouts (as described in subsequent sections). The reconstructed model included 681 metabolic genes, 1436 reactions and 1474 metabolites. The model has been made publicly available in SBML format at

Figure 1 represents the overlap between the reactions and metabolites present in the Methylocella model and those in 2 previously reconstructed models of type II methanotrophs (Methylocystis hirsuta and Methylocystis parvus) [15, 16], as well as the typical scale-free topology of the metabolic network.

Fig. 1

Venn diagrams showing the overlap between the reactions (a) and metabolites (b) present in the reconstructed GSMMs of Methylocella silvestris, Methylocystis parvus and Methylocystis hirsuta. The plot (c) shows the logarithm of the metabolite connectivity (k, the number of reactions in which a metabolite takes part) versus the logarithm of the number (n) of metabolites with connectivity k. The plot shows a typical scale-free topology with a negative slope of 2.5 and an overrepresentation of highly connected metabolites such as ATP and redox co-factors

Differences between the predicted metabolic networks of Methylocella and Methylocystis species

A complete list of reactions and metabolites specific to Methylocella silvestris is provided as Additional file 1: SF1. Among its specific reactions, the metabolic network of Methylocella silvestris contains those catalyzed by the enzymes isocitrate lyase (EC; Msil_3157) and malate synthase (EC; Msil_1325), which form the glyoxylate shunt, allowing the use of ethanol and acetate as sole carbon sources. Other type II methanotrophs such as Methylocystis sp. SB2 and Methylocystis hirsuta [15, 22] can grow on acetate and/or ethanol, however they do not utilize the glyoxylate shunt but rely on the ethylmalonyl pathway (which is absent in Methylocella silvestris) and have very low specific growth rates (0.08 ± 0.006 day−1 for acetate grown M. hirsuta versus 0.05 ± 0.001 h−1 for Methylocella silvestris grown on acetate [12]). The role of isocitrate lyase in the growth of Methylocella silvestris using ethane and acetate, and also growth on C1 compounds, will be discussed in detail in the following section.

Among the metabolites specific to Methylocella silvestris and absent in both of the Methylocystis species considered, we predicted 6-phosphogluconate and its derivatives 6-phosphogluconate-1–5-lactone and 2-keto-3-deoxy-6-phosphogluconate, which are involved in the Entner-Doutdoroff pathway. Other specific metabolites are 4-hydroxy-2-oxovalerate and 2-keto-4-pentenoate, which are linked to the presence of a 2-keto-4-pentenoate hydratase (EC; Msil_1477).

Metabolic roles for isocitrate lyase (ICL) and malate synthase (MS)

Methylocella, compared to other methanotrophs, is characterized by its metabolic versatility and the high variety of substrates on which it can grow. In particular, its use of alkanes such as ethane and propane [8] is of great interest. The ability to grow on ethane and its metabolic intermediates ethanol and acetate can be explained by the presence of ICL and MS.

In order to confirm the activity of these enzymes, enzyme assays were carried out with extracts of acetate grown Methylocella silvestris (see Materials and methods). The measured activities were 23.2 ± 3.3 and 424 ± 59 nmol min−1 mg-protein−1 for ICL and MS respectively. The metabolic model was used to simulate growth on acetate by setting the specific growth rate equal to its experimental value of 0.05 h−1 and minimizing the acetate uptake rate (which is equivalent to a yield optimization). The predicted metabolic fluxes are 0.78 and 0.71 mmol h−1 g-DW−1 for ICL and MS. Enzymatic activities are reported in nmol min−1 mg-Protein−1. Thus, to compare the predicted metabolic fluxes with the results of enzyme activity tests, we need to transform grams of dry weight into milligrams of protein. Assuming that half of the total biomass corresponds to proteins, the predicted in-vivo activities of these enzymes are equivalent to 26 and 24 nmol min−1 mg-Protein−1. The predicted activity of ICL is close to the measured activity (26 versus 23 nmol min−1 mg-Protein−1), whilst the measured activity of MS is one order higher than the minimal activity necessary to support the observed growth rate (424 versus 24 nmol min−1 mg-Protein−1).

Deletion mutants ΔICL and ΔMS for M. silvestris were constructed (see Materials and methods). As expected, both mutants lost the ability to grow on acetate and ethanol. Interestingly, the ΔICL strain also lost its ability to grow on C1 substrates, while the strain ΔMS retained this ability. This suggests that ICL is also playing an anaplerotic role in the serine cycle for the assimilation of C1 compounds. In previous metabolic models of Methylocystis strains [15, 16] this anaplerotic role was filled by a glycine synthase that transforms methylene-tetrahydrofolate into glycine (even though this has not been confirmed experimentally). The phenotypic observations for ΔICL and ΔMS suggest that in Methylocella silvestris, ICL performs this anaplerotic role by supplying the glyoxylate produced to the serine cycle (Figs. 2). Figure 3 shows the effects of deleting ICL and MS respectively.

Fig. 2

Metabolic flux distributions (fluxes in mmol h−1 g-DW−1) predicted by the model for growth on acetate (a) and methane (b). As shown in (b), MS activity is not required for growth on C1 substrates (methane, methanol and methylamine), which is consistent with the ability of ΔMS to grow on these substrates. The figure shows only the main metabolic fluxes relevant for our discussion. The depicted metabolites are also consumed and produced by other metabolic reactions

Fig. 3

a Growth curves of the wild type and ΔICL on succinate; acetate and methanol, ΔICL stops growing on acetate and methanol while keeps its ability to grow on succinate. b Growth curves of the mutant ΔMS; only growth on acetate is affected by the deletion of MS

The role of ICL in supplying glyoxylate to the serine cycle was further confirmed by the fact that addition of glyoxylate to the growth medium rescued the ability of the cells to grow on C1 compounds (Fig. 4b).

Fig. 4

a Growth curves of the wild type and ΔICL on methylamine; ΔICL lost its ability to grow on C1 compounds. b The ability of ΔICL to grow on C1 compounds is rescued by adding glyoxylate to the medium, however Methylocella silvestris is not able to grow on glyoxylate

Qualitative model predictions. Growth on different substrates of the wild type and deletion mutants

Methylocella silvestris has been shown to grow on a broad scope of substrates [8], while it cannot grow on substrates such as glyoxylate, oxalate, glycine or urea. Figure 5 summarizes the different substrates on which the wild type grows.

Fig. 5

Schematic representation of the central carbon metabolism of Methylocella silvestris and the carbon sources in which it grows

Table 1 represents the ability of the wild type and the mutants ΔICL and ΔMS to grow on 12 different substrates predicted by the model. The model predictions match the experimental observations in all the cases.

Table 1 Growth on different carbon sources

Quantitative predictions

Biomass yields on methane and ethanol (Fig. 6) were obtained by monitoring over time biomass growth and substrate consumption, and calculating the slope of biomass produced versus substrate consumed (see Materials and methods). Maximal theoretical yields were obtained by constraining the substrate uptake rate and maximizing the production of biomass. No ATP maintenance consumption was introduced in the simulations; therefore, the results represent the maximal theoretical value. The difference between the theoretical and the experimental values can be explained by ATP maintenance requirements of 3.45 mmol h−1 g-DW−1. The estimated value for Methylocystis hirsuta was 1.25 mmol h−1 g-DW−1 [15].

Fig. 6

a Theoretical maximal yields versus measured yields on methane and ethanol; error bars are standard deviations (n = 3). bBiomass produced versus consumed substrate for one of the replicates

The yield of Methylocella silvestris on methane is lower, both theoretically and experimentally, than those of Methylocystis species [15]. Experimental yields on methane were 5.2 ± 0.17 g-DW mol−1 for Methylocella silvestris versus 7.7 ± 0.26 g-DW mol−1 for Methylocystis hirsuta. The metabolic model predictions are 6.64 and 8 g-DW mol−1 respectively. The difference between both strains is in part related to the redox cofactors used by sMMO and pMMO, with sMMO using NADH, while the pMMO, characteristic of Methylocystis, uses ubiquinone [15], which itself is reduced in complex I of the respiratory chain coupled to proton extrusion, contributing in this way to higher ATP production.

Propane degradation pathways

Two reactions have been incorporated into the model, with respective identifiers “PrMO” (yielding 1-propanol) and “PrMO2” (yielding 2-propanol). Even if some cross activity is possible, the reaction “PrMO” has been annotated as catalyzed by the enzyme PrMO, while the reaction “PrMO2” has been annotated as catalyzed by the enzyme sMMO. Both monooxygenation reactions are coupled to the consumption of an oxygen molecule and the oxidation of an NADH equivalent. M. silvestris grows on both 1-propanol and 2-propanol, although 1-propanol appears to have toxic effects and growth on this substrate is observed only for inocula pre-cultured with propane, but not with other substrates [8]. Growth on 2-propanol was observed in all the cases, independently of the substrate on which the cells were precultured.

The genome of M. silvestris contains eight genes predicted to encode NAD(P)-dependent alcohol dehydrogenases (ADHs), as well as a pyrroloquinoline quinone (PQQ)-containing methanol dehydrogenase (Msil_0471) and a PQQ-containing ADH with 73% identity to xoxF from Methylobacterium extorquens (Msil_1587). For modelling purposes, it is essential to elucidate if the oxidation of 1-propanol and 2-propanol, to propanal and acetone respectively, is coupled to NAD(P)H generation, or coupled to transfer of electrons to PQQ, which are further transferred to cytochrome-c, with proton extrusion [14]. Oxidation by PQQ-containing dehydrogenases was confirmed by assaying the rate of dichlorophenolindophenol reduction in extracts of propane grown cells (using spectrophotometric measurements). Both 1-propanol and 2-propanol were oxidized at similar rates, while NAD and NADP coupled oxidation rates were negligible in both substrates (Table2).

Table 2 Quinoprotein, NAD and NADP-dependent activities (± standard deviations with triplicate measurements) in cell extracts, measured in nmol min−1 mg-protein−1

Methylocella silvestris can grow on both acetone and propanal (the oxidation products of 2-propanol and 1-propanol). The genome revealed the presence of genes encoding a putative pathway from propanal to methylmalonyl-CoA, composed of four reactions with two putative enzymes for each of them (Fig. 7). The existence of this pathway was further supported by the higher activity of methylmalonyl-CoA metabolism in propane-grown cells of Methylocella silvestris revealed by proteomics [23].

Fig. 7

Two alternative metabolic pathways for propane oxidation

The genome annotation did not reveal all the enzymes catalyzing the reactions involved in the downstream metabolism of acetone. Both 2-propanol and acetone accumulated in the culture broth, during growth on propane, which suggests a kinetic bottleneck downstream of acetone. The RAST annotation shows the presence of three putative hydroxyacylglutathione hydrolases (EC; Msil_1898, 0771 and 1051) and three putative lactoylglutathione lyases (EC; Msil_3783, 1643 and 0199). These reactions would allow the transformation of 2-oxopropanal into lactate, which could be further metabolized via its transformation into pyruvate by a putative lactate dehydrogenase present in the genome (Msil_2429, 2430, 2431). However, the enzymes involved in the transformation of acetone to 2-oxopropanal remain to be elucidated. Proteomics has revealed strong overexpression of the gene Msil_1641, induced by propane. This gene has been annotated as a glucose-methanol-choline oxidoreductase, which does not suggest any specific association with propane degradation, therefore its role in M. silvestris was tested experimentally by constructing a Δ1641 mutant. The deletion mutant showed a lower specific growth rate on propane (0.0075 ± 0.0003 h−1 versus 0.0174 ± 0.0002 h−1 for the wild type), which confirmed its relation to propane utilization. More interestingly, when growing on propane, the Δ1641 strain started accumulating acetol in its growth medium (besides 2-propanol and acetone, which also accumulated in the wild type strain). The mutant strain also lost its ability to grow on 2-propanol and acetone, which confirms the involvement of Msil_1641 in the downstream degradation pathway of acetone. Based on the evidence alone (and its annotation by RAST as a NAD associated oxidoreductase), it was assumed that Msil_1641 catalyzes the oxidation of acetol to 2-oxopropanal with concomitant NADH production. The oxidation of acetone to acetol was proposed to be catalyzed by two putative cytochrome P450 oxidoreductases represented in the genome (Msil_0731 and Msil_1926). Similar enzymes have shown to catalyze this reaction in rabbit [24]. This reaction is coupled to oxygen consumption and oxidation of ferredoxin as it is shown in Fig. 8.

Fig. 8

Growth curves on propane of the wild type and the Δ1641 mutant (a). Accumulation of 2-propanol, acetone and acetol in the growth medium, for the wild type and the Δ1641 mutant (b)

Quantitative aspects of propane utilization

There are two alternative pathways for propane degradation in M. silvestris, one of them, via 1-propanol, transforms propane into methylmalonyl-CoA, while a second pathway, via 2-propanol, transforms propane into lactate. Both pathways co-exist simultaneously and the metabolic flux going through each of them depends on the ratio between 1-propanol and 2-propanol produced by PrMO and sMMO [8]. Deletion of the gene Msil_1641 truncated the second pathway and led to the accumulation of 2-propanol, acetone and acetol. Batch experiments, in which Δ1641 was grown in serum flasks with 20% propane in the headspace, revealed a specific growth rate of 0.0075 ± 0.0003 h−1 and specific production rates of 2-propanol, acetone and acetol of respectively: 0.188, 0.075 and 0.152 mmol h−1 g-DW−1. This rate of 0.152 mmol h−1 g-DW−1 was assumed to be equal to the rate of acetol oxidation to 2-oxopropanal in the wild type.

The wild type, which showed a growth rate on propane of 0.0174 ± 0.0002 h−1, produced 2-propanol and acetone at 0.189 and 0.073 mmol h−1 g-DW−1 respectively (with no acetol accumulation in the medium). These experimental values, as well as the acetol oxidation rate of 0.153 mmol h−1 g-DW−1, inferred from the behaviour of Δ1641, were imposed as constraints in the metabolic model. Propane uptake rate was minimized, leading to a prediction of 0.67 mmol h−1 g-DW−1. This corresponds to a biomass yield on propane equal to 25 g-DW mol−1, which is very close to the experimental yield measured for the wild type of 24 ± 2 g-DW mol−1 [8]. This yield was reduced to around one third in the ΔPrMO mutant [8], which is consistent with a higher fraction of propane being transformed to 2-propanol and metabolized through a less efficient metabolic pathway.

Integration of proteomic data

Proteomic data for Methylocella silvestris have been obtained for growth on methane, succinate and propane [23]. The proteome was characterized using reversed phase Ultra-high Pressure Liquid Chromatography (UPLC) prior to mass spectrometric analysis. The numbers of detected proteins (for the most sensitive experimental replicas) were respectively: 672 for cells grown on propane, 802 for cells grown on succinate and 684 for cells grown on methane. Among these proteins, the following numbers of metabolic enzymes (included in the model) were found: 213 for propane, 263 for succinate and 221 for methane.

The reconstructed model was used to calculate correlation coefficients between the predicted metabolic fluxes in each to the three experimental conditions and the enzyme abundances. This allows to identify metabolic reactions whose predicted fluxes correlate with the abundances of the enzymes catalyzing them (or in other words, it aims at finding enzymes with high metabolic control coefficients). Using the terminology of Metabolic Control Analysis (MCA) [25], some enzymes have high metabolic control coefficients, which are defined as the derivatives of the logarithm of the enzyme reaction rate with respect to the logarithm of the enzyme concentration, (a control coefficient of one would mean a linear correlation between the enzyme abundance and the rate of the reaction that it catalyzes) while others have low control coefficients (changes in its abundance have a low impact on the rate of the reactions that they catalyze, a control coefficient of zero meaning an absence of correlation between enzyme abundance and metabolic flux). These control coefficients are properties of the whole metabolic network and cannot be inferred from the kinetics of single enzymes alone. Note that the control coefficient of an enzyme is unrelated to the absolute value of its metabolic flux or to the magnitude of its kinetic constants. It is rather related to the change of metabolic flux caused by changes in its abundance.

These enzymes are responsible for the transcriptional adaptation of the cell to different carbon sources. Model predictions were carried out by setting specific growth rates to their experimental values and minimizing the carbon source uptake rate. In the case of propane, the fluxes in the pathway via lactate (discussed in the previous section), were also constrained to their experimental values. Pearson correlation coefficients and p values were obtained for each of the metabolic enzymes detected in the proteome. The p-vales were corrected for multiple testing and a false discovery rate of 0.05 was set as a cutoff. Nine proteins passed this threshold, among them the three subunits of PrMO, which are expressed only in presence of propane. Two other enzymes were expressed only under growth on propane, those were the previously discussed oxidoreductase coded by the gene Msil_1641, and the methylmalonyl-CoA mutase coded by Msil_3785. The identified enzymes included also two enzymes of the serine cycle, namely phosphoenolpyruvate carboxylase (Msil_1718) and serine-glyoxylate aminotransferase (Msil_1714), which show their highest expression levels during growth on methane. 3-oxoacyl-synthase (Msil_2205) and inorganic pyrophosphatase (Msil_1025) showed their highest expression and metabolic flux during growth on succinate, followed by growth on propane and methane.

Figure 9a shows a plot of the Pearson correlation coefficients between protein expression and predicted reaction rates in each of the three conditions, versus minus the logarithm of the p value resulting from the correlation. Figure 9b illustrates the protein abundances measured under the three studied conditions and the metabolic fluxes in the corresponding reactions predicted by the model (for 6 of the better correlated enzymes).

Fig. 9

a Pearson correlation coefficients and p values for each metabolic enzyme, the red points represent those with a false discovery rate below 0.05 after correcting for multiple testing. b Protein abundances (left side axis) and predicted metabolic fluxes in mmol h−1 g-DW−1 (right side axis) for 6 of the significantly correlated enzymes


In this work we present the first GSMM of an organism of the genus Methylocella. The model captures the metabolic versatility of the strain and is able to reflect its ability to grow on a broad range of substrates as well as to predict quantitatively its biomass yields on methane and ethanol. The model also predicts the phenotypes of two deletion mutants, ΔICL and ΔMS, and could explain the reliance of M. silvestris on the glyoxylate shunt for growth on C1 substrates. This feature makes M. silvestris different from other type II methanotrophs and should be taken in account for the design of future metabolic engineering strategies. Regarding the ability of M. silvestris to grow on propane, two alternative pathways have been identified. Experimental evidence suggests that both pathways operate in parallel. One of the pathways proceeds through methylmalonyl-CoA while the other proceeds through lactate. The existence of 2 independent pathways for propane assimilation makes M. silvestris a potential platform to synthesize compounds using propane as a carbon and energy source. For example, the deletion of lactate dehydrogenase can be expected to disrupt the second pathway and to result in lactate accumulation, while energy and biomass could still be obtained via the first pathway. Alternatively, the second pathway could be disrupted downstream of methylmalonyl-CoA and its metabolic flux deviated to compounds having methylmalonyl-CoA as precursor, while the cell could still use the pathway via lactate to obtain energy and biomass precursors.

Materials and methods

Reconstruction of the Genome Scale Metabolic Model

The genome of Methylocella silvestris BL2 was obtained from the Joint Genome Institute (JGI) (DSM 15510). After annotation with RAST [20] a draft model was generated using SEED [21]. The gene identifiers used in the text correspond to the original annotation, in order to maintain consistence with previous literature, however the model has been constructed based on the RAST annotation provided as Additional file 2: SF2. Additional file 3: SF3 contains the equivalences between the identifiers of both annotations. The draft model was manually curated following the steps previously described [15], which involved reviewing all the genes annotated as having enzymatic activities and checking that they are associated to the correct reactions in the model, correcting the reversibility of reactions in order to avoid thermodynamically unfeasible production of ATP or extrusion of protons, as well as correcting the stoichiometries of some reactions, in particular those involved in the respiratory chain. Some RAST annotations were corrected using genetic evidence, for example the genes Msil_1649, 1650 and 1651 were annotated by RAST as sMMO sub-units, while it had been previously shown experimentally that they encode a propane monooxygenase that cannot oxidize methane [8]. The genetic evidence previously discussed also shows that Msil_1641, which had been annotated by RAST as a glucose-methanol-choline oxidoreductase, is in fact responsible for the oxidation of acetol.

The reconstructed GSMM in SBML format (Methylocella.xml), together with tab separated files containing metabolites (Methylocella_metabolites.txt) and reactions (Methylocella_reactions.txt) and a file containing the top connected metabolites in the model (MethylocellaMets.txt), as well as the RAST annotation in Excel format (Methylocella.xls), can be downloaded from

Enzyme activity tests

Isocitrate lyase and malate synthase (experiments on acetate) were assayed following the method of Dixon and Kornberg [26], adapted for a 1 ml volume. For isocitrate lyase, the reaction mixture contained; potassium phosphate buffer pH 7.0 (final concentration 100 mM), MgCl2 (6 mM), phenylhydrazine HCl (4 mM) L-Cysteine HCl (12 mM) protein (50—200 µg) and was initiated with DL-isocitrate (trisodium salt) (8 mM). Increase in absorbance at 324 nm, due to the accumulation of glyoxylate phenylhydrazone, was recorded against reactions containing water instead of isocitrate. After a lag of approximately 1–2 min, the reaction was linear for at least 10 min. Rates were calculated using ε324 for glyoxylate phenylhydrazone of 1.7 × 104 M−1 cm−1. Malate synthase was assayed by following the decrease in absorbance at 232 nm due to the breakage of the acetyl-CoA thio-ester bond in the presence of glyoxylate. Reactions (1 ml) contained Tris buffer pH 8.0 (final concentration 90 mM), MgCl2 (3.4 mM), acetyl-CoA (sodium salt) (0.05 mM) and protein (100 µg). Absorbance was measured for 5 min before and after addition of glyoxylate (final concentration 0.5 mM). Without substrate, change in absorbance was less than 0.0008 min−1. Rates were calculated using ε232 for acetyl-CoA of 4.5 × 103 M−1 cm−1. Alcohol dehydrogenase (experiments on propane) was assayed as previously described [8]. Protein concentration was measured using Bio-Rad Protein Assay reagent, following the manufacturer’s instructions.

Construction of mutant strains

Unmarked deletion mutants of isocitrate lysase, malate synthase and Msil_1641 were constructed by double homologous recombination, followed by removal of the antibiotic cassette, as previously described [12]. Upstream and downstream regions were generated by PCR, using primers 3157Af / 3157Ar (5′-TCACTGTGCGGCGACTATG-3′ / 5′-TATCGGTACCCGTTGAGGACCGCCTCAAG-3′) and 3157Bf / 3157Br (5′-TATCACGCGTTGCGTCTGCCTTGTTCAGTC-3′ / 5′-TATCGAGCTCCCAGCGCCAGCTGTTCTTC-3′) or 1325Af / 1325Ar (5′-ATCAGTTAACGCCGTGTCGACGCTTATC-3′ / 5′-ATCAGAGCTCCAACCCAGACGCCAAATG-3′) and 1325Bf / 1325Br (5′-ATCAAGATCTGCCAAGCTGGCGTTACCC-3′ / 5′-ATCAGGTACCCGAACGGCTACACGGAAGG-3′), or1641Af / 1641Ar (5′-ATCAGAGCTCAAAGCACGGCCGCTATCG-3′ / 5′-ATCAACGCGTGCGCTTTCGCCCTGATAACC-3′) and 1641Bf / 1641Br (5′-ATCAGGTACCCGTCATTGGGCAACGATAAG-3′ / 5′-GAAACCGCCAATGCATCTC-3′), and cloned into the EcoR1/KpnI and MluI/SacI, or HpaI/SacI and BglII/KpnI, or SacI/MluI and KpnI/EcoRI sites of pCM184 [27], for isocitrate lyase (Msil_3157), malate synthase (Msil_1325) or Msil_1641, respectively.

Growth of M. silvestris on different substrates

Methylocella silvestris BL2 and the three marker-free deletion mutants, were grown in 120 ml serum vials, sealed with rubber stoppers, on dilute nitrate mineral salts medium (DNMS) as previously described [12]. Liquid and solid substrates were added to 5 mM, except monomethylamine (10 mM) and methanol and ethanol (0.1% v/v). Gaseous substrates (methane and propane) were added by injection through the rubber stopper to headspace concentrations of 10 or 20% v/v, and their consumption was monitored by gas chromatography (GC) [8]. For cultures on propane, 2-propanol, acetone and acetol were quantified by GC following solvent extraction as previously described [8]

Measurement of biomass yields

Methane, ethanol and biomass concentrations were monitored over time and the yields were calculating by plotting the produced biomass versus the consumed substrate and obtaining the slope (before reaching limitation by nitrogen). Methane was added to cultures by injection through the rubber stopper to a headspace concentration of 10% v/v, and monitored by gas chromatography (GC) [8]. The initial concentration of ethanol in the medium was 4 mM. Its concentration was quantified by GC, by comparison with standards prepared in water. Culture medium (1 ml) was centrifuged (16,000 × g, 10 min) and 3 μl of the supernatant injected into an Agilent 7890A gas chromatograph fitted with an HP-PLOT Q column (30 m × 530 μm, Agilent, catalogue number 19095P-QO4). Biomass was calculated from optical density (OD540), measured with a Shimadzu UV-1800 spectrophotometer, based on the conversion factor 1 OD ml unit = 0.25 mg dry weight. Methane was measured using a Porapak Q column (Supelco).

Availability of data and materials

All the data have been made available at:


  1. 1.

    Abbasi T, Tauseef SM, Abbasi SA. Anaerobic digestion for global warming control and energy generation, an overview. Renew Sustain Energy Rev. 2012;16:3228–422.

    CAS  Article  Google Scholar 

  2. 2.

    Ocko IB, Hamburg SP, Jacob DJ, Keith DW, Keohane NO, Oppenheimer N, Roy-Mayhew JD, Schrag DP, Pacala SW. Unmask temporal trade-offs in climate policy debates. Science. 2017;356:492–3.

    CAS  Article  Google Scholar 

  3. 3.

    Etiope G, Lassey KR, Klusman RW, Boschi E. Reappraisal of the fossil methane budget and related emission from geologic sources. Geophys Res Lett. 2008;35:L09307.

    Article  Google Scholar 

  4. 4.

    Osborn SG, Vengosh A, Warner NR, Jackson RB. Methane contamination of drinking water accompanying gas-well drilling and hydraulic fracturing. Proc Natl Acad Sci USA. 2011;108:8172–6.

    CAS  Article  Google Scholar 

  5. 5.

    Cantera S, Bordel S, Lebrero R, Gancedo J, García-Encina PA, Muñoz R. Bio-conversion of methane into high profit margin compounds: an innovative, environmentally friendly and cost-effective platform for methane abatement. World J Microbiol Biotechnol. 2019;35:16.

    Article  Google Scholar 

  6. 6.

    Comer AD, Long MR, Reed JL, Brian FP. Flux balance analysis indicates that methane is the lowest cost feedstock for microbial cell factories. Metab Eng Commun. 2017;5:26–33.

    Article  Google Scholar 

  7. 7.

    Dedysh SN, Knief C, Dunfield PF. Methylocella species are facultatively methanotrophic. J Bacteriol. 2005;187:4665–700.

    CAS  Article  Google Scholar 

  8. 8.

    Crombie AT, Murrell JC. Trace-gas metabolic versatility of the facultative methanotrophs Methylocella silvestris. Nature. 2014;510:148–51.

    CAS  Article  Google Scholar 

  9. 9.

    Rahman MT, Crombie A, Chen Y, Stralis-Pavese N, Bodrossy L, Meir P, McNamara NP. Environmental distribution and abundance of the facultative methanotroph Methylocella. ISME J. 2011;5:1061–6.

    CAS  Article  Google Scholar 

  10. 10.

    Farhan Ul, Haque M, Crombie AT, Ensminger SA, Baciu C, Murrell JC. Facultative methanotrophs are abundant at terrestrial natural gas seeps. Microbiome. 2018;6:118.

    Article  Google Scholar 

  11. 11.

    Mason OU, Hazen TC, Borglin S, Chain PS, Dubinsky EA, Fortney JL, Han J, Holman HY, Hultman J, Lamendella R, Mackelprang R, Malfatti S, Tom LM, Tringe SG, Woyke T, Zhou J, Rubin EM, Jansson JK. Metagenome, metatranscriptome and single-cell sequencing reveal microbial response to Deepwater Horizon oil spill. ISME J. 2012;6:1715–27.

    CAS  Article  Google Scholar 

  12. 12.

    Crombie A, Murrell JC. Development of a system for genetic manipulation of the facultative methanotroph Methylocella silvestris BL2. In: Rosenzweig AC, Ragsdale SW, editors. Methods in enzymology. Burlington: Academic Press; 2011. p. 119–133.

    Google Scholar 

  13. 13.

    de la Torre A, Metivier A, Chu F, Laurens LML, Beck DAC, Pienkos PT, Lindstrom ME, Kaluzhnaya MG. Genome-scale metabolic reconstruction and theoretical investigation of methane conversión in Methylomicrobium buryatense strain 5G(B1). Microb Cell Fact. 2015;14:188.

    Article  Google Scholar 

  14. 14.

    Akberdin IR, Thompson M, Hamilton R, Desai N, Alexander D, Henard CA, Guarnieri MT, Kalyuzhnaya MG. Methane utilization in Methylomicrobium alcaliphilum 20ZR: a systems approach. Sci Rep. 2018;8:2512.

    Article  Google Scholar 

  15. 15.

    Bordel S, Rodríguez Y, Hakobyan A, Rodríguez E, Lebrero R, Muñoz R. Genome scale metabolic modeling reveals the metabolic potential of three Type II methanotrophs of the genus Methylocystis. Metab Eng. 2019;54:191–9.

    CAS  Article  Google Scholar 

  16. 16.

    Bordel S, Rojas A, Muñoz R. Reconstruction of a Genome Scale Metabolic Model of the polyhydroxybutyrate producing methanotroph Methylocystis parvus OBBP. Microb Cell Fact. 2019;18:104.

    Article  Google Scholar 

  17. 17.

    Theisen AR, Ali MH, Radajewski S, Dumont MG, Dunfield PF, McDonald IR, Dedysh SN, Miguez CB, Murrell JC. Regulation of methane oxidation in the facultative methanotroph Methylocella silvestris BL2. Mol Microbiol. 2005;58:682–92.

    CAS  Article  Google Scholar 

  18. 18.

    Kalyuzhnaya MG, Puri AW, Lidstrom ME. Metabolic engineering in methanotrophic bacteria. Metab Eng. 2015;29:142–52.

    CAS  Article  Google Scholar 

  19. 19.

    Colby J, Stirling DI, Dalton H. The soluble methane mono-oxygenase of Methylococcus capsulatus (Bath). Its ability to oxygenate n-alkanes, n-alkenes, ethers, and alicyclic, aromatic and heterocyclic compounds. Biochem J. 1977;165:395–402.

    CAS  Article  Google Scholar 

  20. 20.

    Overbeek R, Begley T, Butler RM, Choudhuri JV, Chuang HY, Cohoon M, de Crécy-Lagard V, Diaz N, Disz T, Edwards R, Fonstein M, Frank ED, Gerdes S, Glass EM, Goesmann A, Hanson A, Iwata-Reuyl D, Jensen R, Jamshidi N, Krause L, Kubal M, Larsen N, Linke B, McHardy AC, Meyer F, Neuweger H, Olsen G, Olson R, Osterman A, Pornov V, Pusch GD, Rodionov DA, Rückert C, Steiner J, Stevens R, Thiele I, Vassieva O, Ye Y, Zagnitko O, Vonstein V. The subsystems approach to genome annotation and its use in the project to annotate 1000 genomes. Nucleic Acids Res. 2005;33:5691–702.

    CAS  Article  Google Scholar 

  21. 21.

    Overbeek R, Olson R, Pusch GD, Olsen GJ, Davis JJ, Disz T, Edwards RA, Gerdes S, Parrello B, Shukla M, Vonstein V, Wattam AR, Xia F, Stevens R. The SEED and the rapid annotation of microbial genomes using subsystems technology (RAST). Nucleic Acids Res. 2014;42:D206–D214214.

    CAS  Article  Google Scholar 

  22. 22.

    Im J, Lee SW, Yoon S, DiSprito AA, Semrau JD. Characterization of a novel facultative Methylocystis species capable of growth on methane, acetate and ethanol. Environ Microbiol Rep. 2011;3:174–81.

    CAS  Article  Google Scholar 

  23. 23.

    Patel NA, Crombie A, Slade SE, Thalassinos K, Hughes C, Connolly JB, Langridge J, Murrell JC, Scrivens JH. Comparison of one- and two-dimensional liquid chromatography approaches in the label-free quantitative analysis of Methylocella silvestris. J Proteome Res. 2012;11:4755–63.

    CAS  Article  Google Scholar 

  24. 24.

    Koop DR, Casazza JP. Identification of ethanol-inducible P-450 isozyme 3a as the acetone and acetol monooxygenase of rabbit microsomes. J Biol Chem. 1985;260:13607–12.

    CAS  PubMed  Google Scholar 

  25. 25.

    Kacser H, Burns JA. The control of flux. Symp Soc Exp Biol. 1973;27:65–104.

    CAS  PubMed  Google Scholar 

  26. 26.

    Dixon GH, Kornberg HL. Assay methods for key enzymes of the glyoxylate cycle. Biochem J. 1959;72:3P.

    Google Scholar 

  27. 27.

    Marx CJ, Lidstrom ME. Broad-host-range cre-lox system for antibiotic marker recycling in gram-negative bacteria. Biotechniques. 2002;33:1062–7.

    CAS  Article  Google Scholar 

Download references


This work was performed with the support of the Marie Curie grant H2020-MSCA-IF-2016 CH4BioVal (GA nº 750126). The financial support from the Regional Government of Castilla y León and the FEDER program is also gratefully acknowledged (CLU 2017–09 and VA281P18). We also thank the Spanish Ministry of Economy and Competitiveness, the European FEDER program and the European Commission (CTM2015-73228-JIN). Work on this project was supported by the Leverhulme Trust Research project (grant number RPG2016-050) to JCM and Leverhulme Trust Early Career Fellowship (grant number ECF2016-626) to ATC.


This work was performed with the support of the Marie Curie grant H2020-MSCA-IF-2016 CH4BioVal (GA nº 750126). The financial support from the Regional Government of Castilla y León and the FEDER program is also gratefully acknowledged (CLU 2017-09 and VA281P18).

Author information




SB constructed the models and wrote the article; AC carried out the experiments, read and corrected the manuscript; RM red and corrected the manuscript; CM supervised the work, red and corrected the manuscript. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Sergio Bordel.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher's Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Additional file 1: FS1.

List of unique reactions and unique metabolites in the model of M. Sylvestris.

Additional file 2: FS2.

Gene annotation obtained using RAST.

Additional file 3: FS3.

Equivalence between gene annotations.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Bordel, S., Crombie, A.T., Muñoz, R. et al. Genome Scale Metabolic Model of the versatile methanotroph Methylocella silvestris. Microb Cell Fact 19, 144 (2020).

Download citation