Open Access

Expanding the range of polyhydroxyalkanoates synthesized by methanotrophic bacteria through the utilization of omega-hydroxyalkanoate co-substrates

Contributed equally
AMB Express20177:118

DOI: 10.1186/s13568-017-0417-y

Received: 15 February 2017

Accepted: 28 May 2017

Published: 5 June 2017


The first methanotrophic syntheses of polyhydroxyalkanoates (PHAs) that contain repeating units beyond 3-hydroxybutyrate and 3-hydroxyvalerate are reported. New PHAs synthesized by methanotrophs include poly(3-hydroxybutyrate-co-4-hydroxybutyrate) (P(3HB-co-4HB)), poly(3-hydroxybutyrate-co-5-hydroxyvalerate-co-3-hydroxyvalerate) (P(3HB-co-5HV-co-3HV)), and poly(3-hydroxybutyrate-co-6-hydroxyhexanoate-co-4-hydroxybutyrate) (P(3HB-co-6HHx-co-4HB)). This was achieved from a pure culture of Methylocystis parvus OBBP where the primary substrate is methane and the corresponding ω-hydroxyalkanoate monomers are added as a co-substrate after the cells are subjected to nitrogen-limited conditions.


Methane Methanotroph PHA Biopolymer Copolymer Omega hydroxy acids


Polyhydroxyalkanoates (PHAs) are microbial storage polymers accumulated by many different groups of bacteria as an intracellular carbon and energy reserve. PHAs are biodegradable, biocompatible, and renewable bioplastics (Myung et al. 2014) that could substitute for petrochemical-derived plastics in many applications. Accumulation of PHAs occurs when bacterial cells grow under conditions where substrates other than the electron donor (typically the carbon source), such as nitrogen or phosphorus, limit growth. Depending upon the carbon co-substrates supplied during this nutrient-limited period, PHAs with different compositions are produced. Over one hundred different carboxylic acid monomers are reported to be incorporated into PHAs, resulting in polymers with a wide range of material properties (Steinbüchel and Gorenflo 1997).

Among the variety of polymers produced, 4-hydroxybutyrate (4HB) homopolymer or its copolymer are of interest for various biomedical applications (Martin and Williams 2003). It is a strong, flexible thermoplastic material that can be processed easily to form scaffolds, heart valves, or cardiovascular tissue supports (Martin and Williams 2003). In addition, 4HB polymer is extremely well tolerated in vivo because biological hydrolysis of 4HB homopolymer or copolymer yields 4HB, which is a common metabolite in the human body (Nelson et al. 1981). A copolymer of 3-hydroxybutyrate (3HB) and 4HB units is degradable by lipase and PHA depolymerase, in contrast to most PHAs, which cannot be degraded by lipase (Saito and Doi 1994; Wu et al. 2009). Aside from 4HB, the presence of structurally similar monomer units such as 5-hydroxyvalerate (5HV) and 6-hydroxyhexanoate (6HHx) in PHAs also adds elasticity to the polymer and enhances lipase-mediated degradation of the polymer (Mukai et al. 1993).

Use of methane (CH4) as a feedstock for PHA production can significantly decrease costs and environmental impacts (Rostkowski et al. 2012; Strong et al. 2015). Methane is currently widely available as the major component of natural gas and biogas obtained from the anaerobic degradation of organic waste. When CH4 is the sole feedstock, high molecular weight poly(3-hydroxybutyrate) (P3HB) is the sole PHA product (Wendlandt et al. 2001; Pfluger et al. 2011; Pieja et al. 2011; Myung et al. 2015b, 2016b). Recently, we reported production of poly(3-hydroxybutyrate-co-3-hydroxyvalerate) (PHBV) copolymer by a methanotrophic enrichment (Myung et al. 2015a) and a pure culture of obligate Type II methanotrophs (Myung et al. 2016a) when fed CH4 as a primary feedstock and valerate as a co-substrate.

In general, bacterial enzymes involved in PHA synthesis have broad substrate specificity (Poirier et al. 1995). For example, in Alcaligenes eutrophus, the PHA synthase can incorporate 3-hydroxyvalerate (3HV), 4HB, 4-hydroxyvalerate, 5HV, and 4-hydroxyhexanoate into PHAs (Haywood et al. 1989; Valentin et al. 1992, 1994). To our knowledge, this same broad specificity for substrates was not known for methanotrophic bacteria. Herein, we report the first methanotrophic synthesis of PHAs that contain repeating units beyond 3HB and 3HV, including poly(3-hydroxybutyrate-co-4-hydroxybutyrate) (P(3HB-co-4HB)), poly(3-hydroxybutyrate-co-5-hydroxyvalerate-co-3-hydroxyvalerate) (P(3HB-co-5HV-co-3HV)), and poly(3-hydroxybutyrate-co-6-hydroxyhexanoate-co-4-hydroxybutyrate) (P(3HB-co-6HHx-co-4HB)). This was achieved by a pure culture of Methylocystis parvus OBBP when the primary substrate is CH4 and the corresponding ω-hydroxyalkanoate monomers are added as co-substrates.

Materials and methods

Culture conditions

Unless otherwise specified, all Methylocystis parvus OBBP cultures were grown in medium JM2, which is a modified version of ammonium mineral salts (AMS) medium (Whittenbury et al. 1970). Medium JM2 contained the following chemicals per L of solution: 2.4 mM MgSO4·7H2O, 0.26 mM CaCl2, 36 mM NaHCO3, 4.8 mM KH2PO4, 6.8 mM K2HPO4, 10.5 μM Na2MoO4·2H2O, 7 μM CuSO4·5H2O, 200 μM Fe-EDTA, 530 μM Ca-EDTA, 5 mL trace metal solution, and 20 mL vitamin solution. The trace stock solution contained the following chemicals per L of solution: 500 mg FeSO4·7H2O, 400 mg ZnSO4·7H2O, 20 mg MnCl2·7H2O, 50 mg CoCl2·6H2O, 10 mg NiCl2·6H2O, 15 mg H3BO3 and 250 mg EDTA. The vitamin stock solution contained the following chemicals per L of solution: 2.0 mg biotin, 2.0 mg folic acid, 5.0 mg thiamine·HCl, 5.0 mg calcium pantothenate, 0.1 mg vitamin B12, 5.0 mg riboflavin and 5.0 mg nicotinamide.

All cultures were incubated in 160 mL serum bottles (Wheaton, Millville, NJ, USA) capped with butyl-rubber stoppers and crimp-sealed under a CH4:O2 headspace (molar ratio 1:1.5; >99% purity; Praxair Technology, Inc., Danbury, CT, USA). The liquid volume was 50 mL, and the headspace volume was 110 mL. Cultures were incubated horizontally on orbital shaker tables at 150 rpm. The incubation temperature was 30 °C.

Synthesis of ω-hydroxyalkanoate monomers

The general preparation is a modification of a literature method (Takashima et al. 2004): a 20 mL vial was charged with 6 mL of a 4 M aqueous solution of sodium hydroxide. 2 g of the lactone was slowly added, and the contents stirred for 24 h. Volatiles were then evaporated, and the residue washed. The resulting white powders were dried overnight.

4-Hydroxybutanoate (4-hydroxybutyrate) (from γ-butyrolactone). 78% yield

1H-NMR (Additional file 1: Figure S1a, 500 MHz, D2O) δ 3.54 (t, J = 7.8, 2H), 2.18 (t, J = 8.6, 2H), 1.69–1.60 (m, 2H). 13C-NMR (Additional file 1: Figure S1b, 125 MHz, D2O) δ 183.7, 62.1, 34.6, 29.0. This is in agreement with the literature (Rival et al. 2012).

5-Hydroxypentanoate (5-hydroxyvalerate) (from δ-valerolactone) 72% yield

1H-NMR (Additional file 1: Figure S2a, 500 MHz, DMSO-d6) δ 3.33 (t, J = 6.4 Hz, 2H), 1.88 (dd, J = 8.3, 5.9 Hz, 2H), 1.53–1.29 (m, 4H). 13C-NMR (Additional file 1: Figure S2b, 125 MHz, DMSO-d6) δ 177.8, 60.5, 38.0, 33.9, 22.6. This is in agreement with the literature (Takashima et al. 2004).

6-Hydroxyhexanoate (from ε-caprolactone) 74% yield

1H-NMR (Additional file 1: Figure S3a, 500 MHz, D2O) δ 3.55 (t, J = 6.6 Hz, 2H), 2.14 (t, J = 7.4 Hz, 2H), 1.57–1.46 (m, 4H), 1.32–1.25 (m, 2H). 13C-NMR (Additional file 1: Figure S3b, 125 MHz, D2O) δ 184.0, 61.6, 37.5, 31.0, 25.6, 24.9. This is in agreement with the literature (Lemoine et al. 2014).

Alternatively, the sodium ω-hydroxyalkanoate monomers can be prepared in situ by dissolving 1 g of lactone in approximately 2.5 mL of 4 M aqueous sodium hydroxide and adjusting the pH to 7.

Balanced growth phase and unbalanced PHA production phase

Fifty-milliliter Methylocystis parvus OBBP cultures were grown to final optical densities (OD600) of 0.8–1.2 then centrifuged (3000g) for 15 min. The pellets were resuspended in 30 mL of JM2 medium to create the inoculum for triplicate 160 mL serum bottle cultures. Each culture received 10 mL inoculum plus 40 mL of fresh medium (39.5 mL of medium JM2 plus 0.5 mL of 1.35 M ammonium chloride stock) and was flushed for 5 min with a CH4/O2 mixture (molar ratio of 1:1.5). After growth at 30 °C for 24 h, the headspace in each culture was again flushed for 5 min with the CH4/O2 mixture then incubated at 30 °C for a second 24 h period of balanced growth.

After 48 h, all cultures were harvested and subjected to nitrogen-limiting conditions. Triplicate samples were centrifuged (3000g) for 15 min and suspended in fresh medium without nitrogen. The headspace of each bottle was flushed with the CH4:O2 gas mixture at t = 0 h and t = 24 h. To assess the effects of co-substrate addition of PHA synthesis, the medium was amended with varying concentrations of 4HB, 5HV, and 6HHx monomers. Other organic acid co-substrates including 3HB, butyrate, valerate, hexanoate, and octanoate (Sigma-Aldrich, St Louis, MO, USA) were also tested for PHA copolymer synthesis. After 48 h of incubation, cells were harvested by centrifugation (3000g) and freeze-dried. Preserved samples were assayed for PHA content.

PHA weight percentages

To determine PHA weight percent, between 5 and 10 mg of freeze-dried biomass were weighed then transferred to 12 mL glass vials. Each vial was amended with 2 mL of methanol containing sulfuric acid (3%, vol/vol) and benzoic acid (0.25 mg/mL methanol), supplemented with 2 mL of chloroform, and sealed with a Teflon-lined plastic cap. All vials were shaken and then heated at 95–100 °C for 3.5 h. After cooling to room temperature, 1 mL of deionized water was added to create an aqueous phase separated from the chloroform organic phase. This was mixed on a vortex mixer for 30 s then allowed to partition until phase separation was complete. The organic phase was aspirated by syringe and analyzed using a gas chromatograph (Agilent 6890N; Agilent Technologies, Palo Alto, CA, USA) equipped with an HP-5 column (containing (5% phenyl)-methylpolysiloxane; Agilent Technologies, Palo Alto, CA, USA) and a flame ionization detector. dl-3-Hydroxybutyric acid sodium salt (Sigma-Aldrich, St Louis, MO, USA) and was used to prepare external calibration curves. The PHA content (wt%, wP3HB/wCDW) of the samples were calculated by normalizing to initial dry mass.

Analytical methods

To analyze concentrations of CH4 and O2, 0.5 mL of gas phase from each enrichment culture was injected onto a GOW-MAC gas chromatograph with an Alltech CTR 1 column and a thermal conductivity detector. The following method parameters were used: injector, 120 °C; column, 60 °C; detector, 120 °C; and current, 150 mV. Peak areas of CH4 and O2 were compared to standards and quantified using the software ChromPerfect (Justice Laboratory Software, Denville, NJ, USA).

Concentrations of organic acids were determined using a Dionex DX-500 ion chromatograph (Dionex, Sunnyvale, CA, USA) equipped with a GP50 gradient pump, CD25 conductivity detector, AS40 Automated Sampler, an AS11-HC ion-exchange column, and eluted with a mobile phase containing sodium hydroxide using Chromeleon software (Dionex, Sunnyvale, CA, USA). Organic acids were qualified and quantified using pure standards (HPLC grade).

To analyze total suspended solids (TSS), 0.5–5.0 mL of cell suspension was filtered through pre-washed, dried, and pre-weighed 0.2 μm membrane filters (Pall, Port Washington, NY, USA). The filtered cells and membrane filters were dried at 105 °C for 24 h, then weighed on an AD-6 autobalance (Perkin Elmer, Norwalk, CT, USA).

Material characterization


PHA granules were extracted from the cells by suspending 500 mg of freeze-dried cell material in 50 mL Milli-Q water, adding 400 mg of sodium dodecyl sulfate (>99.0% purity; Sigma-Aldrich, St. Louis, MO, USA) and 360 mg of EDTA, followed by heating to 60 °C for 60 min to induce cell lysis. The solution was centrifuged (3000g) for 15 min, and the pellet washed three times with deionized water. To purify the PHA, pellets were washed with a 50 mL sodium hypochlorite (bleach) solution (Clorox 6.15%), incubated at 30 °C with continuous stirring for 60 min, then centrifuged (3000g) for 15 min. Sample pellets were washed and re-centrifuged three times with deionized water.

Molecular weight

Molecular weights of PHAs were evaluated using gel permeation chromatography (GPC). Sample pellets were dissolved in chloroform at a concentration of 5 mg/mL for 90 min at 60 °C,  filtered through a 0.2 μm PTFE filter, and then analyzed with a Shimadzu UFLC system (Shimadzu Scientific Instruments, Columbia, MD, USA) equipped with a Shimadzu RID-10A refraction index detector. The GPC was equipped with a Jordi Gel DVB guard column (500 Å, Jordi Labs, Mansfield, MA, USA) and Jordi Gel DVB analytical columns (105 Å, Jordi Labs, Mansfield, MA, USA). The temperature of the columns was maintained at 40 °C, and the flow rate of the mobile phase (chloroform) was 1 mL min-1. Molecular weights were calibrated with polystyrene standards from Varian (Calibration Kit S-M2-10, Agilent Technologies, Palo Alto, CA, USA).

Melting temperature

Melting temperatures (Tm), the apparent heat of fusion (ΔHm, the energy required to change a substance from the solid to the liquid state without changing its temperature), and the glass transition temperatures (Tg, the temperature at which the transition in the amorphous regions between the glassy and rubbery state occurs) of PHAs were evaluated using TA Q2000 differential scanning calorimetry (DSC; TA Instruments, New Castle, DE, USA). Thermal data were collected under a nitrogen flow of 10 mL min-1. About 5 mg of melt-quenched PHA samples encapsulated in aluminum pans were heated from −40 to 200 °C at a rate of 10 °C min−1. The melting temperatures were determined from the position of the endothermic peaks. The apparent heat of fusion (ΔHm) was determined from the DSC endothermal peaks in the second scan. The glass transition temperature (Tg) was taken as the inflection point of the specific heat increment at the glass–rubber transition.

Nuclear magnetic resonance (NMR)

1H-NMR spectra (400, 500, and 600 MHz) were recorded at room temperature, with shifts reported in parts per million downfield from tetramethylsilane and referenced to the residual solvent peak. 13C-NMR spectra (100 and 125 MHz, 1048 scans, delay time (d1) = 0.5 s) of PHAs were recorded at room temperature, with shifts reported in parts per million downfield from tetramethylsilane. PHA samples for NMR were prepared by adding approximately 3 mg of the PHA to 0.7 mL deuterated chloroform (CDCl3), with gentle heating until the PHA had dissolved.

Preparations of PHA thin films

In order to produce solution-cast films ~150 µm thick, 0.4 g of bioplastic powder was added to 20 mL of chloroform (ACS reagent grade; ACROS Organics, Morris Plains, NJ, USA). The chloroform and bioplastic were stirred while being heated at the boiling point of chloroform (61 °C) for 2 h, until the bioplastic was completely dissolved. A reflux condenser was used to prevent excessive evaporation of the chloroform. After full dissolution, the liquid was poured into a 60 mm diameter glass petri dish and covered to allow the chloroform to slowly evaporate over 24 h. As noted by Bergstrand (2012), drying rate is a critical parameter for attaining homogeneous films. The optimal evaporation rate was observed when the gap between the lid and the place was between 0.3 and 0.6 mm. Dried films of all bioplastics easily separated from the glass dish and were further trimmed to specimen sizes appropriate for testing. Plastic films were stored at −15 °C until testing to minimize aging effects (Srubar et al. 2012).

Tensile properties

Young’s modulus (E, a measure of stiffness of an elastic material), tensile strength (σt, the resistance of a material to a force tending to tear it apart, measured as the maximum tension the material can withstand without tearing), and elongation at break (εb; the ratio between changed length and initial length after breakage of the test specimen) were determined using an Instron 5565 Universal Testing Machine (Instron Corp., Canton, MA, USA). The dimensions of the specimens were 25 mm × 5 mm × 0.1 mm. The testing conditions used were: cross head speed of 5 mm min-1 and load cell of 0.1 kN.

Statistical sequence analysis of P(3HB-co-4HB)

The method used is described by Doi et al. (1990). 13C-NMR spectroscopy (125 MHz, 6800 scans, delay time (d1) = 5 s, room temperature) was conducted on a P(3HB-co-4HB) sample (Additional file 1: Figure S10) with the fraction of 3HB units, F(3HB), equal to 0.9141 and fraction of 4HB units, F(4HB), equal to 0.0859 (obtained from integration of 1H-NMR spectra). For a statistically random copolymer, Bernoullian statistics can be applied to calculate the expected fractions of diad sequences F(3HB)(3HB), F(3HB)(4HB), F(4HB)(3HB), and F(4HB)(4HB): F(3HB)(3HB) = F (3HB) 2 , F(3HB)(4HB) = F(4HB)(3HB) = F(3HB)(1–F(3HB)), and F(4HB)(4HB) = F (4HB) 2 . Observed diad, triad and tetrad fractions (via peak integration on the 13C-NMR spectrum) were compared to the calculated diad, triad and tetrad fractions for a statistically random copolymer with F(3HB) = 0.9141 and F(4HB) = 0.0859. Finally, the parameter D, which describes the randomness of the polymer chain (with D = 1.0 for a statistically random copolymer), was calculated using the equation D = F(3HB)(3HB)F(4HB)(4HB)/F(3HB)(4HB)F(4HB)(3HB).


Production of two/three component copolymers using various organic acid co-substrates

Table 1 summarizes PHA copolymer production results for M. parvus OBBP. Integration of 1H-NMR spectra was used to determine monomer compositions. When grown with CH4 alone (Additional file 1: Figure S4), P3HB (42 ± 3 wt%) was the sole product. When 1.2 mM of butyrate (Additional file 1: Figure S5) or 3HB (Additional file 1: Figure S6) was added to harvested cells (without nitrogen in the incubation medium), P3HB was again the sole product. The P3HB content ranged from 55 ± 3 to 59 ± 5 wt%. When 1.2 mM of 4HB was added as co-substrate (Fig. 1), 4HB units were incorporated. The wt% P(3HB-co-4HB) was 50 ± 4 wt%, and the mol% 4HB was 9.5 mol%. When 1.2 mM of valerate was added as co-substrate (Additional file 1: Figure S7), 3HV units were incorporated. The wt% PHBV was 54 ± 4 wt%, and the mol% 3HV was 25.0 mol%. When 1.2 mM of 5HV was added as a co-substrate (Fig. 2), 5HV and 3HV units were incorporated, forming a three-component PHA. The mol% 5HV was 3.6 mol% and the mol% 3HV was 1.5 mol%. When 1.2 mM of hexanoate was added (Additional file 1: Figure S8), P3HB was the sole product. The wt% P3HB was 56 ± 4 wt%. When 1.2 mM of 6HHx was added as a co-substrate (Fig. 3), 6HHx and 4HB units were incorporated, forming a three-component PHA. The mol% 6HHx was 1.4 mol% and the mol% 4HB was 1.0 mol%. When 1.2 mM of octanoate was added (Additional file 1: Figure S9), P3HB was the sole product. The wt% P3HB was 54 ± 3 wt%. In all cases, the primary substrate was CH4. In the absence of CH4, no PHA was synthesized, an observation consistent with our previous observation that CH4 oxidation is required for methanotrophic PHA synthesis (Myung et al. 2016a).
Table 1

PHA production using various fatty acid co-substrates by M. parvus OBBP


wt% PHA polymer

PHA monomer ratio (mol%)

TSS (mg/L)







42 ± 3






1600 ± 180

Butyrate (1.2 mM)

55 ± 3






1660 ± 200

3-Hydroxybutyrate (1.2 mM)

59 ± 5






1820 ± 220

4-Hydroxybutyrate (1.2 mM)

50 ± 4






1720 ± 240

Valerate (1.2 mM)

54 ± 4






1760 ± 160

5-Hydroxyvalerate (1.2 mM)

48 ± 4






1640 ± 180

Hexanoate (1.2 mM)

56 ± 4






1740 ± 200

6-Hydroxyhexanoate (1.2 mM)

48 ± 3






1680 ± 220

Octanoate (1.2 mM)

54 ± 3






1720 ± 180

Fig. 1

1H-NMR spectrum of P(3HB-co-4HB) produced by M. parvus OBBP

Fig. 2

1H-NMR spectrum of P(3HB-co-5HV-co-3HV) produced by M. parvus OBBP

Fig. 3

1H-NMR spectrum of P(3HB-co-6HHx-co-4HB) produced by M. parvus OBBP

Influence of 4HB concentrations on P(3HB-co-4HB) production

To understand the effect of co-substrate on product formation, a range of 4HB concentrations were added, and the mol% 4HB in P(3HB-co-4HB) was monitored (Fig. 4). For added 4HB levels <1 mM, the mol% 4HB of the PHA copolymer increased with increasing 4HB concentrations. At higher levels, the 4HB fraction stabilized at ~10 mol%.
Fig. 4

4HB fractions in P(3HB-co-4HB) produced relative to initial 4HB concentrations. The primary carbon substrate is CH4. The errors bars represent standard deviations for triplicate batch cultures

Molecular weight characterization

Table 2 illustrates the number average molecular weights (Mn) and the molecular weight distributions (Mw/Mn; a measure of the distribution of molecular mass in a given polymer sample) of PHAs produced by M. parvus OBBP. The Mn of all PHAs tested were above 1.0 × 106 Da, indicating production of PHAs with high molecular weights. These values are comparable to those of heterotrophic enrichments and to commercial P3HB and PHBV powders (Table 2, Sigma-Aldrich, St Louis, MO, USA) (Myung et al. 2014), but are more uniform, with higher Mn and lower Mw/Mn.
Table 2

Physical properties of the methanotroph produced PHA polymers

PHA products

Molecular weights

Thermal properties

Mechanical properties



Tm (°C)

ΔHm (J/g)

Tg (°C)

E (GPa)

σt (MPa)

εb (%)


1.48 E+06








P(3HB-co-24 mol% 3HV)

1.32 E+06








P(3HB-co-3.0 mol% 4HB)

1.33 E+06








P(3HB-co-9.5 mol% 4HB)

1.22 E+06








P(3HB-co-3.6 mol% 5HV-co-1.4 mol% 3HV)

1.26 E+06








P(3HB-co-1.4 mol% 6HHx-co-1.0 mol% 4HB)

1.27 E+06








Commercial P3HB

7.38 E+05



Commercial PHBV

4.48 E+05



M n number average molecular weight, M w weight average molecular weight, T m melting temperature, ΔH m apparent heat of fusion, T g glass transition temperature, E Young’s modulus, σ t tensile strength, ε b elongation at break

Melting temperatures of the PHA generated

The thermal behaviors of the two/three component PHA copolymers were investigated using differential scanning calorimetry (DSC) (Table 2). The melting temperature (Tm) of P3HB was highest at 178 °C and were lower for the two/three component PHA copolymers tested, ranging from 135 to 148 °C. The apparent heat of fusion (ΔHm) was highest at 83 J/g and were the two/three component PHA copolymers tested, ranging from 44 J/g to 65 J/g. The glass transition temperature (Tg) of P3HB was highest at 3 °C and were lower for the two/three component PHA copolymers tested, ranging from −5 to −1 °C.

Mechanical properties of the produced PHA copolymers

Table 2 illustrates the mechanical properties of thin-film PHA samples determined using Instron Universal Testing Machine. P3HB had the highest Young’s modulus (E) of 3.0 GPa, and the other PHA copolymers had significantly lower Young’s modulus ranging from 0.7 to 1.2 GPa. The tensile strength (σt) was also highest for P3HB at 43.2 MPa, and the tensile strengths of other PHA copolymers tested ranged from 22.0 to 35.6 MPa. However, elongation at break (εb) was greatly improved from 5.2% to 50.5–284% upon copolymerization.

Statistical sequence analysis of P(3HB-co-4HB)

The observed diad fractions of the P(3HB-co-4HB) sample (F(3HB) = 0.9141 and F(4HB) = 0.0859) match closely with calculated diad fractions based on a statistically random copolymer obeying Bernoullian statistics (Additional file 1: Table S1). The value of the parameter D, calculated using the carbonyl peaks of the 13C-NMR spectrum, was 1.29. This is close to the value of D for a statistically random copolymer (D = 1.0).


Our group and others have previously reported production of P3HB and PHBV by pure culture methanotrophs using CH4 and various co-substrates (Cal et al. 2016; Flanagan et al. 2016; Myung et al. 2016a). The general rule was that even-numbered carbon co-substrates (e.g. 3HB, crotonate) led to production of P3HB, whereas odd-numbered carbon co-substrates (e.g. propionate, valerate, 2-pentenoate, or pentanol) led to production of PHBV. Depending on the number of carbon atoms, fatty acid substrates are processed via the beta-oxidation pathway into either acetyl-CoA or propionyl-CoA, the precursors of P3HB and PHBV.

Addition of ω-hydroxyalkanoate co-substrates resulted in a different outcome. In this case, M. parvus OBBP synthesized a random copolymer containing 3HB and ω-hydroxyalkanoate monomers. While various species of bacteria have synthesized PHAs containing 4HB or 5HV monomers (Poirier et al. 1995; Chanprateep et al. 2010; Chuah et al. 2013), this is the first report of methane-dependent production of PHA copolymers other than PHBV.

The outcome of ω-hydroxyalkanoate co-substrate addition was dependent upon the presence and position of the hydroxyl group (Fig. 5; Table 1). When butyrate or 3HB was added, P3HB was produced; when 4HB was added, the resulting polymer was P(3HB-co-4HB). When valerate was added, the resulting polymer was PHBV, but when 5HV was added, the product was P(3HB-co-5HV-co-3HV). When hexanoate was added, the polymer product was P3HB, but when 6HHx was added, the product was P(3HB-co-6HHx-co-4HB). From these results, we can conclude that the presence of a hydroxyl group and its position play a key role in determining the composition of the PHA produced. When there is a hydroxyl group on the nth carbon (e.g. ω-hydroxyalkanoates), the co-substrate seems to be incorporated directly into the polymer by PHA synthase (PhaC) (Fig. 6), and it can also undergo beta-oxidation, as evidenced by formation of 4HB monomer units derived from the 6HHx co-substrate.
Fig. 5

Scheme of PHA production using methane and co-substrates. a Without the hydroxyl group and b with the hydroxyl group

Fig. 6

C1-oxidation dependent synthesis of PHAs in serine-cycle methanotrophic bacteria. The bold arrow denotes an acyl-CoA pathway likely activated by ω-hydroxyalkanoate co-substrates

Thermal stability is critical for polymer melt processing. P3HB has a narrow processing window, melting at 175–180 °C and thermally degrading at ~190 °C. PHA copolymers produced by incorporation of ω-hydroxyalkanoate monomers have significantly lower melting temperatures (Tm), expanding the processing window (Table 2). These copolymers also had lower Tg values suggesting increased chain mobility compared to P3HB. This would manifest as a decrease in brittleness, an expectation confirmed by the results of mechanical testing summarized below.

Key mechanical properties for useful application of bioplastics are Young’s modulus (E), tensile strength (σt), and elongation at break (εb). P3HB has high E and σt, but is brittle, with a small εb. Short chain-length monomers generally confer toughness and high crystallinity, and medium chain-length monomers generally confer elasticity and low crystallinity. Thus, a mixture of the two enables production of PHA that is both tough and elastic, an important combination of properties for many applications.

Heterotrophic bacteria have been shown to produce P(3HB-co-4HB) (Doi et al. 1990; Nakamura et al. 1992; Saito and Doi 1994; Chanprateep et al. 2010) and P(3HB-co-5HV-co-3HV) (Doi et al. 1987; Steinbuchel and Valentin 1995), but methanotrophic synthesis of these PHA copolymers has not been reported previously. To the best of our knowledge, this is the first reported microbial synthesis of P(3HB-co-6HHx-co-4HB). Generalizing these results, we envision that control over the structure and concentration of added co-substrates will enable synthesis of copolymers suitable for a broad range of applications (Fig. 4).

Use of CH4 as the primary substrate for PHA synthesis is of interest because CH4 is abundant, cheap, and its use does not adversely impact the food supply, unlike cultivated feedstock (Levett et al. 2016). The cost of ω-hydroxyalkanoate co-substrates is high, but can be significantly reduced when lactones are used as the precursor for chemical synthesis of ω-hydroxyalkanoates (see “Materials and methods” section). We conclude that provision of methane as primary substrate and addition of ω-hydroxyalkanoate as co-substrates is a promising route for synthesis of polymers with tunable physical properties.


























ammonium mineral salts


total suspended solids


gel permeation chromatography


nuclear magnetic resonance


Authors’ contributions

JM and CSC designed and coordinated the study. JM and JCAF carried out the experimental work. JM and JCAF drafted the manuscript. RMW and CSC highly contributed for the manuscript revision. All authors read and approved the final manuscript.


We thank the Stanford Nano Shared Facilities for staff assistance, training, and access to instruments required for this research. We also thank Cecily A. Ryan for help with the preparations of PHA thin films.

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

The datasets supporting the conclusions of this article are included within the article. Methylocystis parvus OBBP is available in publicly accessible culture collection (ATCC® 35066™).


This work was supported by unrestricted gifts from Chevron and a Samsung Scholarship. JF is grateful to the Stanford Center for Molecular Analysis and Design (CMAD) for a graduate fellowship.

Publisher’s Note

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

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.

Authors’ Affiliations

Department of Civil and Environmental Engineering, Stanford University
Department of Chemistry, Stanford University
Woods Institute for the Environment
William and Cloy Codiga Resource Recovery Center
Department of Civil and Environmental Engineering, Pennsylvania State University
Brighton College


  1. Bergstrand A (2012) Preparation of porous poly(3-hydroxybutyrate) films by water-droplet templating. J Biomater Nanobiotechnol 3:431–439View ArticleGoogle Scholar
  2. Cal AJ, Sikkema WD, Ponce MI, Franqui-Villanueva D, Riiff TJ, Orts WJ, Pieja AJ, Lee CC (2016) Methanotrophic production of polyhydroxybutyrate-co-hydroxyvalerate with high hydroxyvalerate content. Int J Biol Macromol 87:302–307View ArticlePubMedGoogle Scholar
  3. Chanprateep S, Buasri K, Muangwong A, Utiswannakul P (2010) Biosynthesis and biocompatibility of biodegradable poly(3-hydroxybutyrate- co-4-hydroxybutyrate). Polym Degrad Stab 95:2003–2012View ArticleGoogle Scholar
  4. Chuah J-A, Yamada M, Taguchi S, Sudesh K, Doi Y, Numata K (2013) Biosynthesis and characterization of polyhydroxyalkanoate containing 5-hydroxyvalerate units: effects of 5HV units on biodegradability, cytotoxicity, mechanical and thermal properties. Polym Degrad Stab 98:331–338View ArticleGoogle Scholar
  5. Doi Y, Tamaki A, Kunioka M, Soga K (1987) Biosynthesis of terpolyesters of 3-hydroxybutyrate, 3-hydroxyvalerate, and 5-hydroxyvalerate in Alcaligenes eutrophus from 5-chloropentanoic and pentanoic acids. Macromol Rapid Commun 8:631–635View ArticleGoogle Scholar
  6. Doi Y, Segawa A, Kunioka M (1990) Biosynthesis and characterization of poly(3-hydroxybutyrate-co-4-hydroxybutyrate) in Alcaligenes eutrophus. Int J Biol Macromol 12:106–111View ArticlePubMedGoogle Scholar
  7. Flanagan JCA, Myung J, Criddle CS, Waymouth RM (2016) Poly(hydroxyalkanoate)s from waste biomass: a combined chemical–biological approach. ChemistrySelect 1:2327–2331View ArticleGoogle Scholar
  8. Haywood GW, Anderson AJ, Dawes EA (1989) The importance of PHB-synthase substrate specificity in polyhydroxyalkanoate synthesis by Alcaligenes eutrophus. FEMS Microbiol Lett 57:1–6View ArticleGoogle Scholar
  9. Lemoine H, Marković D, Deguin B (2014) Mild and chemoselective lactone ring-opening with (TMS)ONa. Mechanistic studies and application to sweroside derivatives. J Org Chem 79:4358–4366View ArticlePubMedGoogle Scholar
  10. Levett I, Birkett G, Davies N, Bell A, Langford A, Laycock B, Lant P, Pratt S (2016) Techno-economic assessment of poly-3-hydroxybutyrate (PHB) production from methane-the case for thermophilic bioprocessing. J Environ Chem Eng 4:3724–3733View ArticleGoogle Scholar
  11. Martin DP, Williams SF (2003) Medical applications of poly-4-hydroxybutyrate: a strong flexible absorbable biomaterial. Biochem Eng J 16:97–105View ArticleGoogle Scholar
  12. Mukai K, Doi Y, Sema Y, Tomita K (1993) Substrate specificities in hydrolysis of polyhydroxyalkanoates by microbial esterases. Biotechnol Lett 15:601–604View ArticleGoogle Scholar
  13. Myung J, Strong NI, Galega WM, Sundstrom ER, Flanagan JCA, Woo SG, Waymouth RM, Criddle CS (2014) Disassembly and reassembly of polyhydroxyalkanoates: recycling through abiotic depolymerization and biotic repolymerization. Bioresour Technol 170:167–174View ArticlePubMedGoogle Scholar
  14. Myung J, Galega WM, Van Nostrand JD, Yuan T, Zhou J, Criddle CS (2015a) Long-term cultivation of a stable methylocystis-dominated methanotrophic enrichment enabling tailored production of poly(3-hydroxybutyrate-co-3-hydroxyvalerate). Bioresour Technol 198:811–818View ArticlePubMedGoogle Scholar
  15. Myung J, Wang Z, Yuan T, Zhang P, Van Nostrand JD, Zhou J, Criddle CS (2015b) Production of nitrous oxide from nitrite in stable Type II methanotrophic enrichments. Environ Sci Technol 49:10969–10975View ArticlePubMedGoogle Scholar
  16. Myung J, Flanagan JCA, Waymouth RM, Criddle CS (2016a) Methane or methanol-oxidation dependent synthesis of poly(3-hydroxybutyrate-co-3-hydroxyvalerate) by obligate type II methanotrophs. Process Biochem 51:561–567View ArticleGoogle Scholar
  17. Myung J, Kim M, Pan M, Criddle CS, Tang SKY (2016b) Low energy emulsion-based fermentation enabling accelerated methane mass transfer and growth of poly(3-hydroxybutyrate)-accumulating methanotrophs. Bioresour Technol 207:302–307View ArticlePubMedGoogle Scholar
  18. Nakamura S, Doi Y, Scandola M (1992) Microbial synthesis and characterization of poly(3-hydroxybutyrate-co-4-hydroxybutyrate). Macromolecules 25:4237–4241View ArticleGoogle Scholar
  19. Nelson T, Kaufman E, Kline J, Sokoloff L (1981) The extraneural distribution of gamma-hydroxybutyrate. J Neurochem 37:1345–1348View ArticlePubMedGoogle Scholar
  20. Pfluger AR, Wu WM, Pieja AJ, Wan J, Rostkowski KH, Criddle CS (2011) Selection of Type I and Type II methanotrophic proteobacteria in a fluidized bed reactor under non-sterile conditions. Bioresour Technol 102:9919–9926View ArticlePubMedGoogle Scholar
  21. Pieja AJ, Rostkowski KH, Criddle CS (2011) Distribution and selection of poly-3-hydroxybutyrate production capacity in methanotrophic proteobacteria. Microb Ecol 62:564–573View ArticlePubMedGoogle Scholar
  22. Poirier Y, Nawrath C, Somerville C (1995) Production of polyhydroxyalkanoates, a family of biodegradable plastics and elastomers, in bacteria and plants. Nat Biotechnol 13:142–150View ArticleGoogle Scholar
  23. Rival N, Hazelard D, Hanquet G, Kreuzer T, Bensoussan C, Reymond S, Cossy J, Colobert F (2012) Diastereoselective synthesis of the C17–C30 fragment of amphidinol 3. Org Biomol Chem 10:9418–9428View ArticlePubMedGoogle Scholar
  24. Rostkowski KH, Criddle CS, Lepech MD (2012) Cradle-to-gate life cycle assessment for a cradle-to-cradle cycle: biogas-to-bioplastic (and back). Environ Sci Technol 46:9822–9829PubMedGoogle Scholar
  25. Saito Y, Doi Y (1994) Microbial synthesis and properties of poly(3-hydroxybutyrate-co-4-hydroxybutyrate) in Comamonas acidovorans. Int J Biol Macromol 16:99–104View ArticlePubMedGoogle Scholar
  26. Srubar WV III, Wright ZC, Tsui A, Michel AT, Billington SL, Frank CW (2012) Characterizing the effects of ambient aging on the mechanical and physical properties of two commercially available bacterial thermoplastics. Polym Degrad Stab 97:1922–1929View ArticleGoogle Scholar
  27. Steinbüchel A, Gorenflo V (1997) Biosynthetic and biodegradable polyesters from renewable resources: current state and prospects. Macromol Symp 123:61–66View ArticleGoogle Scholar
  28. Steinbuchel A, Valentin HE (1995) Diversity of bacterial polyhydroxyalkanoic acids. FEMS Microbiol Lett 128:219–228View ArticleGoogle Scholar
  29. Strong PJ, Xie S, Clarke WP (2015) Methane as a resource: can the methanotrophs add value? Environ Sci Technol 49:4001–4018View ArticlePubMedGoogle Scholar
  30. Takashima Y, Osaki M, Harada A (2004) Cyclodextrin-initiated polymerization of cyclic esters in bulk: formation of polyester-tethered cyclodextrins. J Am Chem Soc 126:13588–13589View ArticlePubMedGoogle Scholar
  31. Valentin HE, Schönebaum A, Steinbüchel A (1992) Identification of 4-hydroxyvaleric acid as a constituent of biosynthetic polyhydroxyalkanoic acids from bacteria. Appl Microbiol Biotechnol 36:507–514View ArticleGoogle Scholar
  32. Valentin HE, Lee Eun Yeol, Choi Cha Yong, Steinbuchel A (1994) Identification of 4-hydroxyhexanoic acid as a new constituent of biosynthetic polyhydroxyalkanoic acids from bacteria. Appl Microbiol Biotechnol 40:710–716View ArticleGoogle Scholar
  33. Wendlandt KD, Jechorek M, Helm J, Stottmeister U (2001) Producing poly-3-hydroxybutyrate with a high molecular mass from methane. J Biotechnol 86:127–133View ArticlePubMedGoogle Scholar
  34. Whittenbury R, Phillips KC, Wilkinson JF (1970) Enrichment, isolation and some properties of methane-utilizing bacteria. J Gen Microbiol 61:205–218View ArticlePubMedGoogle Scholar
  35. Wu Q, Wang Y, Chen GQ (2009) Medical application of microbial biopolyesters polyhydroxyalkanoates. Artif Cells Blood Substit Immobil Biotechnol 37:1–12View ArticlePubMedGoogle Scholar


© The Author(s) 2017