Research article | Open | Published:
Detection of phase-dependent transcriptomic changes and Rubisco-mediated CO2 fixation into poly (3-hydroxybutyrate) under heterotrophic condition in Ralstonia eutropha H16 based on RNA-seq and gene deletion analyses
BMC Microbiologyvolume 13, Article number: 169 (2013)
Ralstonia eutropha H16 is well known to produce polyhydroxyalkanoates (PHAs), which are potential bio-based biodegradable plastics, in an efficient manner as an energy storage material under unbalanced growth conditions. To obtain further knowledge of PHA biosynthesis, this study performed a quantitative transcriptome analysis based on deep sequencing of the complementary DNA generated from the RNA (RNA-seq) of R. eutropha H16.
Total RNAs were extracted from R. eutropha cells in growth, PHA production, and stationary phases on fructose. rRNAs in the preparation were removed by repeated treatments with magnetic beads specific to bacterial rRNAs, and then the 36 bp sequences were determined using an Illumina high-throughput sequencer. The RNA-seq results indicated the induction of gene expression for transcription, translation, cell division, peptidoglycan biosynthesis, pilus and flagella assembly, energy conservation, and fatty acid biosynthesis in the growth phase; and the repression trends of genes involved in central metabolisms in the PHA production phase. Interestingly, the transcription of genes for Calvin-Benson-Bassham (CBB) cycle and several genes for β-oxidation were significantly induced in the PHA production phase even when the cells were grown on fructose. Moreover, incorporation of 13C was observed in poly(3-hydroxybutyrate) synthesized by R. eutropha H16 from fructose in the presence of NaH13CO3, and further gene deletion analyses revealed that both of the two ribulose 1,5-bisphosphate carboxylase (Rubiscos) in CBB cycle were actually functional in CO2 fixation under the heterotrophic condition.
The results revealed the phase-dependent transcriptomic changes and a CO2 fixation capability under heterotrophic conditions by PHA-producing R. eutropha.
Ralstonia eutropha H16, a Gram-negative facultative chemolithoautotrophic bacterium, can utilize various organic compounds such as sugars, organic acids, fatty acids, and plant oils in the heterotrophic growth mode, while in the absence of organic substrates, it thrives autotrophically on H2 and CO2 as the energy and carbon sources, respectively, where CO2 is fixed by Calvin-Benson-Bassham (CBB) cycle . This strain has been also known to accumulate poly(3-hydroxybutylate) [P(3HB)] as a storage compound under unbalanced growth conditions, if a carbon source is available in excess while another essential element (N, O, P, S, or metals) is growth limiting at the same time. It has been estimated that P(3HB) accumulation has a role in survival under the stress conditions.
Bacterial P(3HB) has attracted industrial attention because it is a biodegradable thermoplastic that can be produced from renewable carbon sources; thus it is a possible alternative to petroleum-based polymer materials. A number of studies have focused on P(3HB) biosynthesis by R. eutropha H16, particularly regarding the biosynthetic pathways and enzymes, as well as the biogenesis, structure, and mobilization of intracellular P(3HB) granule [2–7]. In this strain, P(3HB) is synthesized from the central intermediate acetyl-CoA through three step reactions catalyzed by β-ketothiolase (PhaA), NADPH-dependent acetoacetyl-CoA reductase (PhaB1), and PHA synthase (PhaC1), the genes of which are clustered in phaC1-A-B1. The intracellular P(3HB) exists as granules coated with a layer of phospholipids and several proteins, i. e. PhaC1, P(3HB) depolymerases (PhaZs) and phasins (PhaPs). The phaC1-A-B1 operon or the respective genes from R. eutropha H16 have been used to confer the capability for P(3HB) biosynthesis to non-PHA-producing bacteria such as Escherichia coli, as well as higher plants . This strain has also been used as a host for metabolic engineering with the aim of biosynthesizing PHA copolyesters with more flexible properties compared with the brittle and hard P(3HB) homopolymer [9–15].
The complete genome analysis of R. eutropha H16 was reported in 2006 . The genome consists of three circular replicons; chromosome 1 (4.05 Mbp), chromosome 2 (2.91 Mbp), and megaplasmid pHG1 (0.45 Mbp); and the genes for essential metabolisms and cellular functions are located on chromosome 1. The genome information has facilitated the genome-wide transcriptome analysis of this strain. Hitherto, transcriptome analyses of R. eutropha were performed using a DNA microarray technique. Peplinski et al. reported a comparison of the transcriptomes of wild-type strain H16 and the two PHA-negative strains in different growth phases based on competitive hybridization . They observed significant differences in the transcription levels of a large number of genes in these strains, including genes involved in lipid metabolisms. However, the comparison of transcriptomes in the exponential growth and P(3HB) biosynthesis phases of R. eutropha was unclear. Brigham et al. carried out a transcriptomic comparison of R. eutropha H16 cells grown in fructose- and trioleate-containing media, and identified two gene clusters responsible for β-oxidation .
Hybridization-based DNA microarray methods have mainly been used for global transcriptome analysis; however, these methods exhibit a relatively low dynamic range for detecting transcription because of two reasons. One is a high level of noise caused by cross-hybridization, and the other is saturation and poor sensitivity at very high and low transcriptional levels, respectively . Recently, the direct sequencing of complementary DNA generated from RNA (RNA-seq) based on high-throughput DNA sequencing technology was often used to study RNA population within the cells . Many studies have demonstrated that RNA-seq has several advantages over the previous microarray methods used for transcriptional analysis, including a larger dynamic range, lower background noise, and greater sensitivity . In addition, this technique enables comparison of the transcription levels of different genes in the same sample. Although RNA-seq was initially difficult to apply to bacterial cells without poly-A tails in their mRNA, enrichment of the mRNA by rRNA pulldown and great improvement in the sequencing depth of the recent sequencer can overcome this problem .
In this study, we applied RNA-seq to profile and quantify the transcription levels of R. eutropha H16 genes in the growth, PHA biosynthesis, and stationary phases on fructose. We successfully detected a number of interesting transcriptomic changes that depended on the cellular phases. Recently, Brigham et al. carried out a microarray analysis of this strain in different phases, and identified the regulation of PHA biosynthesis by a stringent response . Several of our results were consistent with those based on the microarray analysis as described below, and one of the interesting results was a significant induction of CBB cycle in the PHA production phase on fructose. Thus, we investigated the possibility of CO2 fixation during P(3HB) biosynthesis by R. eutropha H16 under heterotrophic conditions, and demonstrated that both of the two ribulose 1,5-bisphosphate carboxylase (Rubisco) in the transcriptionally activated CBB cycle actually played a role in incorporation of 13C into P(3HB) synthesized from fructose in the presence of NaH13CO3.
Result and discussion
Cultivation, sample preparation, and RNA sequencing
R. eutropha H16 was cultivated in a mineral salt medium containing 0.2% (w/v) NH4Cl to separate the PHA production phase from the growth phase precisely. As shown in Figure 1(A), the cells grew initially without PHA biosynthesis and started to accumulate P(3HB) after 18 h of cultivation. P(3HB) was produced up to 42 wt% of dry cell mass during 26–36 h with a nearly constant residual cell mass, and then reached to stationary. Total RNA was isolated from cells in the growth phase at 16 h (referred to as F16), PHA production phase at 26 h (F26), and stationary phase at 36 h (F36) [Figure 1(A)]. When octanoate was supplied as a non-sugar growth substrate, the cell growth and PHA biosynthesis initially occurred simultaneously and further PHA production was observed after the saturation of cell growth [Figure 1(B)]. Therefore, the total RNA was isolated from cells in the PHA production phase not associated with cell growth at 26 h (O26), 2 h after the third stepwise addition of octanoate.
The rRNA in the total RNA was removed repeatedly, and the enriched mRNA was subjected to RNA-seq with two technical replicates. The numbers of mapped reads (36 bp) with no mismatches reached about 26–43 million reads per run (Table 1). Despite the removal of rRNA twice, 72–89% of the reads still mapped to rRNA regions, which indicated that the mRNA enrichment procedure required further optimization. The reads that mapped onto rrn operons (consisting of rrs, tRNA-Ile, tRNA-Ala, rrl, and rrf) were discarded from the set of reads, and the remaining reads were used as the total reads. We obtained 3–10 million reads other than rrn operons that mapped onto the R. eutropha genome, which were considered to be sufficient for transcriptome analysis of the small bacterial genome. The genes with significant changes in expression were used in the subsequent analysis (P < 0.05), i. e. 5,553 genes out of a total 6,635 genes. Of the statistically non-significant genes, over 90% of the genes were silent or had weak expression with reads per kilobase per million mapped reads (RPKM) values of <250 in all of the samples examined.
Overview of R. eutropha transcriptomes
Clustering of the four transcriptomes (F16, F26, F36, and O26) based on the calculated RPKM values detected global changes in the transcription levels of a number of genes, which depended on the cellular phases (Figure 2). However, the clustering analysis indicated the strong resemblance of the O26 transcriptome to that of F36. In particular, there are almost no significant differences between F36 and O26 in terms of the expression levels of genes encoding β-oxidation enzymes, including the two gene clusters previously identified by Brigham et al. . These facts implied that the transcriptional changes related to fatty acid metabolism had already fulfilled 2 h after the stepwise addition of octanoate at 24 h. Thus, the O26 transcriptome was not examined in detail in the present study. Further optimization of the time point for RNA isolation should be considered to obtain the transcriptomes of R. eutropha grown on fatty acids. The medium-chain-length (mcl)-(R)-3-hydroxyacyl-CoA molecules are provided through β-oxidation in several PHA-producing bacteria, including R. eutropha[9, 11–14, 24], therefore, the transcriptomic changes that depended on the chain length of fatty acids would be valuable information.
Table 2 summarizes highly expressed gene clusters during cultivation on fructose (indicated by arrows in Figure 2). Gene clusters that encoded a number of ribosomal proteins and RNA polymerase subunits (H16_A3457-A3484 and H16_A3490-A3505), and membrane-bound hydrogenase subunits along with the accessory proteins (PHG001-PHG023) were highly expressed throughout cultivation. In the growth phase (F16), the expression of gene clusters related to pilus assembly proteins (H16_A0981-A0987), cell-division and peptidoglycan biosynthesis (H16_A3268-A3282), fatty acid biosynthesis (H16_A2560-A2572), ATP synthase subunits (H16_A3636-A3643), and NADH dehydrogenase subunits (H16_A1050-A1063) were high, which are consistent with their importance of cell assembly and energy conservation for cell growth. Interestingly, significant transcriptional induction in the PHA production phase (F26) was observed for the gene clusters H16_A1949-A1957, H16_B1380-B1395 and PHG416-PHG427, of which the latter two clusters contained cbb operons that encode CBB cycle enzymes involved in CO2 fixation (see below).
The highly expressed genes with RPKM values >20,000 in at least one of the three phases in the fructose-containing medium are shown in Additional file 1: Table S1. A number of ribosomal protein genes were well expressed in the growth phase, as well as several transcription and translation factors, groES-EL (H16_A0705-A0706), secY and secE (H16_A3464 and H16_A3503), and such others. The high-level expression of rpoN (H16_A0386) was observed throughout cultivation, which was particularly high in the nitrogen-deficient PHA production phase as expected. H16_A3402, which encodes an outer membrane protein (porin), exhibited the highest RPKM values in F16 and F26; while H16_B2205, which encodes a cold shock protein, exhibited high-level expression throughout cultivation on fructose, particularly in F16.
Additional file 1: Tables S2 and S3 show the highly up-regulated and down-regulated genes in the PHA production phase to the growth phase (F26/F16), respectively. The highly down-regulated genes, i. e. genes with high induction in the growth phase, included flg cluster (H16_B0258-B0271) and two fli clusters (H16_B0561-B0567 and H16_B2360-B2373) related to flagella assembly, as well as several genes in che operon (H16_B0229-B0245) that are related to chemotaxis (Additional file 1: Table S3). Raberg et al. reported that flagellation was strongly occurred during growth and stagnated during PHA biosynthesis . Similar results were obtained in a previous microarray-based comparison of R. eutropha H16 and a PHA-negative mutant PHB-4 .
A recent microarray analysis by Brigham et al. reported that PHB production was regulated by a stringent response, because most of the upstream regions of the strongly up-regulated genes during nitrogen stress contained the consensus elements for σ54-family promoters . Many of the genes were also highly up-regulated by 20–50 fold during the nitrogen-depleted PHA production phase in the present study, such as H16_A0359, H16_A2801, H16_B0780, H16_B0948, and H16_B1156 (Additional file 1: Table S2). A gene cluster that encodes potential nitrogen-scavenging transporters and enzymes (H16_A1075-A1087) was also up-regulated in F26 by 4–16 fold to F16 (data not shown). The expression ratios were much less than 50-491-fold detected in the microarray analysis , but the present RNA-seq analysis supported the expression regulation for these genes by the stringent response.
Transcriptome changes related to major metabolic processes and cellular functions
The genome analysis of R. eutropha H16 has identified three important clusters participated in fructose degradation in chromosome 2. The genes in cluster 1 (H16_B1497-B1503), which are frcRACBK, pgi2, and zwf2 were significantly induced in the growth phase (Figure 3), suggesting the important roles in transportation and conversion of extracellular fructose to 6-phosphogluconolactone for growth. The genes in cluster 2, which are glk, zwf3, pgl, and edd2 (H16_B2564-B2567) have roles in sugar phosphorylation and Entner-Doudoroff (ED) pathway. The expression levels of these genes were low in F16 and F26, and slightly increased in F36. The cluster 3 (H16_B1211-B1213), which consists of a gene of putative 2-amino-2-deoxy-D-gluconate hydrolase and kdgK for glucosaminate degradation, and eda involved in ED pathway, was observed to be induced in the growth phase.
R. eutropha H16 lacks a gene encoding phosphofructokinase ; therefore, Embden-Meyerhof (EM) pathway is assumed to function in conversion of glyceraldehyde 3-phosphate generated via ED pathway into pyruvate, or in gluconeogenesis on non-sugar growth substrates. Of the genes for EM pathway, transcription of gapA (H16_A3146) and eno (H16_A1188) were extensively high in F16. While, reaction steps between 3-phosphoglycerate and fructose-6-phosphate in EM pathway are shared with CBB cycle. R. eutropha possesses two sets of CBB enzymes, which are encoded in cbb c and cbb p operons in chromosome 2 (H16_B1383-B1395) and megaplasmid pHG1 (PHG416-PHG427), respectively . We observed that the two cbb operons were expressed in the growth phase at levels comparable to the genes for ED pathway. Pentose-phosphate cycle is thought to be defective in R. eutropha H16 because of a lack of 6-phosphogluconate dehydrogenase; therefore, several enzymes in CBB cycle would have a role in establishing the non-oxidative branch of pentose-phosphate cycle, along with rpe (H16_A3317), rpiA (H16_A2345), tal (H16_A2346), tktA (H16_A3147) located in loci other than the cbb operons, thereby providing essential precursors for nucleotides and aromatic amino acids. The expression of cbb genes has been known to be activated by a transcriptional regulator CbbR (H16_B1396), which is encoded within cbb c operon  when the intracellular concentration of phosphoenolpyruvate (PEP) becomes low under autotrophic conditions . Several studies have also reported that partial derepression of the cbb genes also occurred during the late growth phase on a few substrates, such as fructose and gluconate [1, 28, 29]. Examination of our RNA-seq revealed that, even with partial derepression, the induction of both of the cbb operons in F26 was significant differences between the transcriptomes in the growth and PHA production phases, as shown in Figures 2 and 3. The previous microarray analyses of R. eutropha also showed that the transcription levels of the cbb operons were higher in the wild-type H16 strain than in a PHA-negative mutant PHB-4 , and they were induced in the absence of nitrogen . PHA biosynthesis from acetyl-CoA may accompany a reduction in the intracellular concentration of PEP, which could lead to the transcriptional activation of the cbb operons.
Pyruvate metabolisms and TCA cycle
E1, E2, and E3 are components of the pyruvate dehydrogenase complex, which are encoded by pdhA1 (H16_A1374), pdhB (H16_A1375), and pdhL (H16_A1377), respectively, and they were highly induced in the growth phase. In particular, pdhL exhibited an 18.5-fold increased expression in the growth phase compared with the PHA production phase, which was consistent with a previous observation that disruption of pdhL decreased the growth rate and PHA productivity on fructose . pdhA2 (H16_A1753) and aceE (H16_B1300), which encode paralogs of PdhA1 and PdhL, respectively, were barely expressed throughout cultivation. gltA (H16_A2627), acnA and acnB (H16_A2638 and H16_B0568, respectively), and icd1 and icd2 (H16_A3056 and H16_B1931, respectively), which encode enzymes for the conversion of C6-acids in TCA cycle, were highly expressed in the growth phase, but had slightly lower expression levels in the PHA production and stationary phases, except for the constitutively transcribed icd2. In addition to gltA, four genes are related to citrate synthase in R. eutropha H16, but we observed weak expression of H16_B2211 and negligible expression of the other three genes. The genes that encode other TCA cycle members also exhibited variable expression. For example, odhABL (H16_A2325-A2323) and sdhCDAB (H16_A2632-A2629) tended to be highly expressed in the growth and PHA production phases, whereas sucCD (H16_A0547-A0548) were induced in the growth phase. The genes for methylcitrate pathway  were constitutively expressed, although the level of expressions were very weak during the cultivation on fructose.
iclA (H16_A2211) and iclB (H16_A2227), both encodes isocitrate lyase in glyoxylate bypass, were observed to be highly induced in the PHA production phase. In particular, the transcription of iclB in F26 increased 33-fold as compared to that in F16. This result suggested a drastic change in the carbon flux from TCA cycle to glyoxylate bypass during PHA biosynthesis, but Brigham et al. have demonstrated that single disruptions of iclA or iclB did not affect the growth and PHA biosynthesis in R. eutropha H16 grown on fructose . pyc (H16_A1251), pepck (H16_A3711) and ppc (H16_A2921) were present in the genome as genes encoding potential enzymes related to anaplerotic formation of oxaloacetate. A previous study reported that transcription and enzyme activities were detected only for pepck among the three genes in R. eutropha, whereas the present RNA-seq results indicated moderate expression of ppc and pepck as well as weak but actual expression of pyc throughout cultivation.
In Escherichia coli during high-cell density cultivation, it has been reported that genes involved in EM pathway and pentose-phosphate cycle were highly expressed in the stationary phase, probably to compensate for the reduced TCA cycle activity . The transcription of genes for ED pathway in Zymomonas mobilis significantly increased under anaerobic ethanol-producing conditions to facilitate energy conservation . In R. eutropha under the PHA biosynthesis condition, we observed a decreasing trend in expression of the genes in ED pathway and TCA cycle. The activity of ED pathway and TCA cycle during the PHA production phase is probably attributable to pre-existing as well as newly synthesized enzymes with the reduced transcription. The probably decreased flux of central metabolisms were supported by our recent metabolomics analysis of R. eutropha H16 that detected lower intracellular concentrations of many sugar phosphates in the PHA production phase than in the growth phase on fructose . It can be assumed that the decreased metabolic activity appeared to be enough to maintain cellular viability and P(3HB) synthesis in a condition not associated with cell growth, as seen in Corynebacterium glutamicum in a glutamate-producing condition .
de novo Fatty acid synthesis and β-oxidation
In R. eutropha H16, accA1, accA2, accB, accC1, accC2, accC3, and accD have been annotated as genes of the acetyl-CoA carboxylase (ACC) subunits. Based on a consideration of the general quaternary structure of ACC and the expression levels of these genes, the major ACC in this strain probably consisted of AccA1 (H16_A1223) as the carboxyl transferase subunit α (CTα), AccD (H16_A2611) as the carboxyl transferase subunit β (CTβ), AccB and AccC2 (H16_A3171-A3172) as the biotin carboxyl carrier protein (BCCP) and biotin carboxylase (BC), respectively. The expression levels of these genes were high in the growth phase, and then slightly decreased in the PHA production phase (Figure 4). accC1 (H16_A0184, BC-BCCP) and H16_A0177 (CTαβ) may be another pair of ACC or the related carboxylase, because these had weak and similar expression behaviors to each other. The expression levels of accA2 (H16_A2142, BC-BCCP) and accC3 (H16_A3290, BC-BCCP-CTαβ) were negligible throughout cultivation on fructose. The genes fabHDG-acpP-fabF (H16_A2569-A2565), fabZ (H16_A2044), and fabI1 (H16_A2410), which are involved in de novo fatty acid biosynthesis, were highly expressed in the growth phase, but many of the genes still had rather high expression levels in the PHA production phase.
A high number of genes in R. eutropha H16 are annotated as enzymes that potentially functions in fatty acid β-oxidation, which indicates the possible versatility of this strain for degradation of various hydrophobic compounds. Based on a detailed domain search, we identified 51 genes for acyl-CoA synthetase (ACS), 54 genes for acyl-CoA dehydrogenase (ACDH), 53 genes for enoyl-CoA hydratase (ECH), 3 genes for 3-hydroxyacyl-CoA dehydrogenase (3HCDH), and 21 genes for β-ketothiolase (KT). In fact, our RNA-seq examination revealed that many genes for putative β-oxidation enzymes were even expressed on fructose, as shown in Figure 4. The previous microarray study revealed that the two gene clusters of H16_A0459-A0464 and H16_A1526-A1531 were induced and in deed played important roles during β-oxidation in the cells grown on trioleate . It was observed that the cluster H16_A0459-A0464 (which contains ACDH, 3HCDH-ECH fusion, KT, and ECH) was expressed weakly throughout cultivation on fructose, while the cluster H16_A1526-A1531 (which contains ECH-3HCDH fusion, KT, and ACDH) exhibited approximately 8.5 to 11.4-fold increased expression in the PHA production phase compared with that in the growth phase. fadD3 (H16_A3288), which has been reported to be induced on trioleate , was moderately and constitutively expressed on fructose. H16_B1148, which encodes another ACS, was extremely induced in the PHA production phase. The cluster H16_A1067-A1070 was also induced in the PHA production phase. In particular, the induction ratio and expression levels of H16_A1067 and A1068, both encoding ACDH, were very high in F26. Both of H16_A1069 and A1070 were identified as genes that encode homologs of (R)-specific enoly-CoA hydratase (R-ECH), and the product of H16_A1069 (PhaJ4a) has been demonstrated to be an R-ECH that is specific to mcl-enoyl-CoAs . These results strongly suggested that fatty acid β-oxidation was functional even in the presence of fructose in R. eutropha H16, and it may have a role in the active turnover of acyl moieties derived from lipids. Tsuge et al. reported that when R. eutropha PHB-4 expressed laboratory-evolved phaC1 from Pseudomonas sp. 61-3, it accumulated PHA co-polyester which contained a small fraction of mcl-3-hydroxyalkanoate units from fructose . It was assumed that the mcl-(R)-3-hydroxyacyl-CoA monomers were provided through the activated β-oxidation linked with lipid turnover when the cells were grown on fructose. The detection of the mcl-CoA-thioesters in R. eutropha H16 cells grown on fructose according to the metabolomic analysis  was consistent with this expectation.
A previous quantitative-real time PCR (qRT-PCR) analysis, which used 16SrRNA as an internal quantification control, reveled that the relative expression levels of phaC1-A-B1 (H16_A1437-A1439) decreased during the growth phase . In contrast, a recent microarray analysis reported similar expression levels of phaC1-A-B1 in conditions with or without a nitrogen source . The RNA-seq analysis in the present study showed rather similar transcription levels of phaA and phaB1, as well as a 3.7-fold induction of phaC1 expression in F26 when compared with F16. These contradictory results may have been caused by the use of different analytical platforms. Thus, we performed a detailed qRT-PCR analysis of phaC1 using the total RNA samples prepared for RNA-seq with three primer sets (shown in Additional file 1: Table S4) and two inner controls (16SrRNA and bfr2 [H16_A0328]). As shown in Additional file 1: Figure S1, when 16SrRNA was used as an inner control, the three amplifications of different phaC1 regions indicated decrease of expression as longer cultivation time, which were in accordance with the previous qRT-PCR result . However, qRT-PCR of N-terminal and central regions of phaC1 with bfr2 control indicated induction of the gene expression in the PHA production phase. It appeared that the induction behavior of phaC1 was feasible, because the induced expression levels of phaC1 in F26 based on qRT-PCR and RNA-seq agreed well with the strong positive correlation of the expression ratios of other genes obtained from different platforms, as shown in Additional file 1: Figure S2.
Of the 21 KT genes, phaA, bktB (H16_A1445), and H16_A0170 have been reported to be the major participants in P(3HB) biosynthesis . The RNA-seq analysis revealed that the expression of bktB and H16_A0170 increased in the PHA production phase (Figure 3). In addition, we detected expression of other KT genes, namely, H16_A0462, H16_A1528, and H16_B0759 (Figure 4). This result coincided with the recent microarray analysis . The former two genes are located within the β-oxidation clusters , which suggests the contribution of their gene products in thiolysis of medium/long-chain-length 3-ketoacyl-CoA intermediates during lipid turnover. Indeed, the disruption of H16_A1528 gave no effect on growth and PHB accumulation when grown on fructose . The expression behaviors of phaB2 (H16_A2002) and phaB3 (H16_A2171), as well as the negligible transcription of the second PHA synthase gene phaC2 (H16_A2003) were well agreed with the previous microarray analyses [17, 22, 38].
The PHA granule-associated proteins, which are known as phasins, are encoded by 7 genes in R. eutropha H16. phaP1 (H16_A1381) encodes a major phasin, and its PHA biosynthesis-coupled induction was reported to be mediated by an autoregulator PhaR (H16_A1440) . In our study, phaP1 had the third highest expression level in F26 (Additional 1: Table S2). Pötter et al. proposed the PhaR-mediated regulation of phaP3, but the down-regulation of phaP3 expression was observed in the PHA production phase. It was reported that PhaP3 was a major phasin in the phaP1-deficient mutant of R. eutropha; therefore, the release of PhaR from the phaP3 region may occur only in the absence of PhaP1. A previous observation suggested that PhaP2 (PHG202) was not present on the granule surface in vivo, whereas the expression level of phaP2 was very high in the growth and PHA production phases. Another study suggested that PhaP2 may have indirectly participated in the formation of P(3HB) granule by interacting with other phasins . In our study, phaP4 (H16_B2021) was expressed during cultivation with the lower level than phaP1 and phaP2. PhaP5 (H16_B1934) , PhaP6 (H16_B1988) and PhaP7 (H16_B2326) , and PhaM (H16_A0141)  were recently identified as new granule-associated proteins, although the expression levels of their corresponding genes were observed to be very low. The weak expression level of phaP5 in F26 markedly contradicted with a previous microarray analysis ; hence, further validation will be necessary.
R. eutropha possesses 5 PHA depolymerases with a DepA domain (phaZ1-Z5), 2 additional depolymerases with an LpqC domain (phaZ6 and phaZ7) and 2 hydroxybutyrate oligomer hydrolases (phaY1 and phaY2) that are considered to be involved in mobilization of P(3HB). Despite the cellular phases examined in the present study were not the PHA utilization phase, the expression levels of phaZ4 (PHG178) and phaY2 (H16_A1335) in the growth phase; and phaZ1 (H16_A1150) and phaZ6 (H16_B2073) in the PHA production phase were rather higher than those of others.
Kaddor et al. demonstrated that the fructose-specific ABC-type transporter FrcACB, which is encoded within the sugar degradation gene cluster 1, was essential for the growth of R. eutropha H16 on fructose . We observed significant down-regulation of these genes in the PHA production phase compared with the growth phase, as described above (Figure 2 and Additional 1: Table S3). The weak expression level of frcACB may be sufficient to support an adequate carbon flux for PHA biosynthesis, or other transporters may have roles in this process. However, the resent microarray analysis reported up-regulation of the fructose transporter genes during nitrogen starvation . copP2 (H16_A3668), which encodes a putative copper uptake P-type ATPase; and nosFD (PHG249-PHG250), which encodes putative copper-specific ABC transporter subunits, were highly up-regulated in the growth phase along with copDCBA (H16_B2182-B2185) and copZ (H16_A3669) (Additional file 1: Table S3), which confer resistance to copper. The up-regulation of these genes was estimated to be due to formation of active copper-containing enzymes, such as cytochrome c oxidase, in an aerobic respiratory chain .
13CO2 Fixation into P(3HB) synthesized from fructose in the presence of NaH13CO3 by R. eutropha H16
It was not clear whether CBB cycle induced under the heterotrophic condition was actually functional in CO2 fixation; therefore, we examined the incorporation of 13C into P(3HB) synthesized by R. eutropha in the presence of NaH13CO3. First, the wild-type H16 strain was cultivated in a nutrient rich medium for cell growth, and P(3HB) biosynthesis was promoted in a nitrogen-free mineral salt medium that contained fructose with periodic additions of NaHCO3 (12C or 13C). It was confirmed that the cell growth was not occurring, but the P(3HB) content was increased from approximately 5 wt% to 50 wt% during the second stage. The abundance of 13C in the P(3HB) fraction after the addition of NaH12CO3 was determined to be 1.13% by gas chromatography–mass spectrometry analysis (GC-MS), which was the same as the natural 13C-abundance (Table 3). Notably, when NaH13CO3 was added to the medium, the abundance of 13C in P(3HB) increased to 2.22%. To elucidate the function of Rubisco(s) in 13CO2-fixation during the heterotrophic PHA production, we performed single and double deletions of the two sets of Rubisco genes [cbbLS c (H16_B1394-B1395) in the cbb c operon and cbbLS p (PHG426-PHG427) in the cbb p operon]. The recombinant strains were cultivated according to the same procedure and analyzed. The results showed that the abundance of 13C in P(3HB) was 1.25% within the double disruptant H16∆∆cbbLS. The slight increase from the natural 13C-abundance was assumed to be caused by anaplerotic carboxylation or other carboxylation reactions. The cultivation of another wild-type strain of R. eutropha JMP134, which lacks Rubisco and ribulose-5-phosphate kinase that are the two key enzymes in CBB cycle, also produced the same results as H16∆∆cbbLS (data not shown). It was calculated that the wild-type H16 strain incorporated 8-fold more 13C into P(3HB) from NaH13CO3 when compared to H16∆∆cbbLS. The abundance of 13C- in P(3HB) synthesized by H16∆cbbLS c and H16∆cbbLS p were 1.81% and 2.11%, respectively, which were slightly lower than the abundance of 13C with H16 strain but higher than that with the double disruptant. Namely, both of the Rubiscos were involved in 13C-incorporation and were able to compensate for the lack of another enzyme to a considerable extent. The results indicated that, even in the heterotrophic condition on fructose, the transcriptionally activated CBB cycle was actually functional in CO2 fixation by R. eutropha H16. This was also supported by our recent detection of ribulose 1,5-bisphosphate, a key metabolite in CBB cycle, based on metabolomic analysis of R. eutropha H16 grown on fructose or octanoate .
This study applied the RNA-seq technique to analyze the genome-wide transcriptional dynamics of PHA-producing R. eutropha H16. The mRNA enrichment using a commercially available probe specific to bacterial rRNA was incomplete for R. eutropha even after two repeated operations, but the greater depth of new sequencing technology could overcome this problem by giving sufficient numbers of reads from mRNA. A comparison of the transcriptomes detected several phase-depending changes in the expression of genes responsible for shifts in the physiological state of R. eutropha throughout cultivation on fructose. In the growth phase, there was high level induction of genes related to transcription, translation, cell division, peptidoglycan biosynthesis, pilus and flagella assembly, energy conservation, and fatty acid biosynthesis; while the genes related to central metabolism were repressed in the PHA production phase. Interestingly, the CBB cycle genes and several β-oxidation genes were transcriptionally activated in the PHA production phase compared with that in the growth phase, when fructose was supplied as the sole carbon source. We further found that 13CO2 was incorporated into P(3HB) when R. eutropha H16 was incubated in the fructose-containing medium in the presence of NaH13CO3. The incorporation of 13C was significantly reduced by the double disruption of both Rubisco genes, which demonstrated that the CO2 fixation was mediated by Rubisco, i.e., the transcriptionally activated CBB cycle was functional during heterotrophic PHA biosynthesis. To the best of our knowledge, this is the first report to demonstrate CO2 fixation into PHA under a heterotrophic condition. The results of our study will facilitate further metabolic engineering of R. eutropha for improved production of PHAs from non-fossil resources, such as the increased metabolic flux from sugars to PHA, the provision of mcl-(R)-3-hydroxyacyl-CoA monomers from sugars through lipid turnover, and fixation of CO2 into the polymer materials.
Cultivation, RNA isolation, and mRNA enrichment
R. eutropha wild strain H16 (DSM428) was cultivated in a 500 ml flask on a reciprocal shaker (115 strokes/min) at 30°C with 100 ml of a nitrogen-limited mineral salts (MB) medium, which was composed of 9 g/l Na2HPO4 · 12H2O, 1.5 g/l KH2PO4, 2.0 g/l NH4Cl, 0.2 g/l MgSO4 · 7H2O, and 1 ml/l trace element solution  in deionized water. A filter-sterilized solution of fructose was added to the medium at a final concentration of 20 g/L. When octanoate was used as a carbon source, 0.1% (w/v) of sodium octanoate (filter-sterilized) was added stepwise at 12 h intervals to avoid the toxic effects on cell growth.
The cells in 10 ml culture broth at 16, 26, and 36 h on fructose and 26 h on octanoate were harvested by centrifugation (1,400 g, 10 min, 4°C), and total RNA was isolated from the cell pellet by using RNeasy Midi Kit (Qiagen, Valencia, CA, USA). RNA eluted in 150 μl RNase-free water was treated with DNase I. 25–50 μg of the total RNA was then subjected to repeated treatment using RiboMinus Transcriptome Isolation Kit (Yeast and Bacteria) (Invitrogen, Carlsbad, CA, USA) for mRNA enrichment. Samples after the treatment were concentrated by ethanol precipitation and dissolved in 30 μl of RNase-free water. The removal of a large fraction of rRNA was confirmed by conventional agarose electrophoresis and ethidium bromide staining, and the quality and quantity of the enriched mRNA samples were assessed by 2100 Bioanalyzer (Agilent Technologies, Santa Clara, CA, USA).
Library construction, sequencing, and data analysis
RNA-seq template libraries were constructed with 1 μg of the enriched mRNA samples using RNA-Seq Template Prep Kit (Illumina Inc., San Diego, CA, USA) according to the manufacturer's instructions. Deep sequencing was performed by Illumina GAIIx sequencer and 36 base-single end reads were generated.
The raw reads were mapped onto genome sequences of R. eutropha H16; NC_008313 (chromosome 1), NC_008314 (chromosome 2), NC_005241 (megaplasmid pHG1), using Burrows-Wheeler Aligner (BWA) . The alignments with mismatch or mapped to the five rRNA regions of R. eutropha H16 (1806458–1811635, 3580380–3575211, and 3785717–3780548 on chromosome 1, and 174896–180063 and 867626–872793 on chromosome 2) were discarded, and the remaining reads were used as total reads. RPKM value (Reads Per Kilobase per Megabase of library size)  for each coding DNA sequence was calculated as a quantitative gene expression index by using custom Perl scripts. For multi-hit reads that did not aligned uniquely, the reciprocal number of the mapped loci was counted for the read. Analysis of variance (ANOVA) of the RPKM values obtained from the two replicates of the samples, and distributed visualization of the significantly changed genes in expression levels (P < 0.05) were performed by using MeV .
R. eutropha cells were harvested by centrifugation (5,000 g, 10 min, 4°C), washed with cold deionized water, centrifuged again, and then lyophilized. Cellular PHA contents were determined by gas chromatography (GC) after methanolysis of the dried cells in the presence of 15% (v/v) sulfuric acid in methanol, as described previously .
Construction of disruption plasmids and strains
A plasmid pK18ms∆cbbLSc for deletion of cbbLS c from chromosome 2 of R. eutropha H16 was constructed as below, and primers are listed in Additional file 1: Table S4. First, upstream and downstream regions (about 1 kbp) of cbbLS c were individually amplified by PCR with genomic DNA of R. eutropha H16 as a template and primer sets of cbbLSc-up5’/cbbLSc-up3’ and cbbLSc-down5’/cbbLSc-down3’, respectively. The second PCR with the amplified fragments using cbbLSc-up5’/cbbLSc-down3’ primers gave a fused fragment of the upstream and downstream regions of cbbLS c . The resulting fragment was digested by EcoRI and HindIII and then ligated with pK18mobsacB  at the corresponding sites to obtain pK18ms∆cbbLSc. pK18ms∆cbbLSp for deletion of cbbLS p from megaplasmid pHG1 was constructed in the same way using primer sets of cbbLSp-up5’/cbbLSp-up3’ and cbbLSp-down5’/cbbLSp-down3’.
Transconjugation of mobilizable plasmids from E. coli S17-1 to R. eutropha and isolation of strains generated by pop in-pop out recombination using the pK18mobsacB-based suicide plasmids were performed as described previously [13, 14]. The strains H16∆cbbLS c , H16∆cbbLS p , and H16∆∆cbbLS were obtained by single deletion of cbbLS c and cbbLS p , and double deletion of the genes in R. eutropha H16, respectively.
Determination of the abundance of 13C in P(3HB)
Cultivation of R. eutropha strains H16, H16∆cbbLS c , H16∆cbbLS p , and H16∆∆cbbLS were done in a 500 ml flask on a reciprocal shaker (115 strokes/min) at 30°C. Firstly, the strains were cultivated in 100 ml of a nutrient rich medium composed of 10 g/l tryptone, 2 g/l yeast extract, and 1 g/l meat extract in tap water for 12 h. The grown cells in 50 ml of the culture broth were harvested, washed with a salt solution (9 g/l Na2HPO4 · 12H2O, 1.5 g/l KH2PO4 in deionized water), and then transferred into 100 ml of a nitrogen-free MB medium (pH6.5 adjusted with KH2PO4) containing 0.5% (w/v) fructose. The cells were further incubated for 24 h to promote P(3HB) biosynthesis. NaH12CO3 (1.08% 13C (natural abundance)) or NaH13CO3 (98% 13C) (Taiyo Nippon Sanso, Tokyo, Japan) was added to a final concentration of 5 mM periodically every 2.5 h during the second stage, taking into consideration loss of dissolved CO2 to the atmosphere.
The cells after the second stage cultivation were harvested, washed, and lyophilized as described above. The dried cells were subjected to methanolysis, and analyzed by GCMS-QC2010 system (Shimadzu, Kyoto, Japan) equipped with an InertCap 1 capillary column (ϕ0.25 mm, 30 m) (GL Science, Tokyo, Japan). 13C/12C ratios in the fragments of CH3–CH=OH+ (m/z 45), CH3–C(OH)H–CH3–C=O+ (m/z 87), and CH3–O–CO–CH2–CH=OH+ (m/z 103) derived from 3HB methyl ester were calculated from the respective isotopomer abundances, and the mean was referred as a abundance of 13C in the P(3HB) fraction.
RNA-seq data accession number
The RNA-seq data used in this study have been deposited in the NCBI Gene Expression Omnibus (GEO) under the accession number of GSE47759.
Bowien B, Kusian B: Genetics and control of CO2 assimilation in the chemoautotroph Ralstonia eutropha. Arch Microbiol. 2002, 178: 85-93. 10.1007/s00203-002-0441-3.
Ishizaki A, Tanaka K, Taga N: Microbial production of poly-D-3-hydroxybutyrate from CO2. Appl Microbiol Biotechnol. 2001, 57: 6-12. 10.1007/s002530100775.
Jendrossek D: Polyhydroxyalkanoate granules are complex subcellular organelles (carbonosomes). J Bacteriol. 2009, 191: 3195-3202. 10.1128/JB.01723-08.
Rehm BHA: Polyester synthases: natural catalysts for plastics. Biochem J. 2003, 376: 15-33. 10.1042/BJ20031254.
Rehm BHA: Biogenesis of microbial polyhydroxyalkanoate granules: a platform technology for the production of tailor-made bioparticles. Curr Issues Mol Biol. 2007, 9: 41-62.
Steinbüchel A, Lütke-Eversloh T: Metabolic engineering and pathway construction for biotechnological production of relevant polyhydroxyalkanoates in microorganisms. Biochem Eng J. 2003, 16: 81-96. 10.1016/S1369-703X(03)00036-6.
Sudesh K, Abe H, Doi Y: Synthesis, Structure and Properties of Polyhydroxyalkanoates: biological Polyesters. Prog Polym Sci. 2000, 25: 1503-1555. 10.1016/S0079-6700(00)00035-6.
Van Beilen JB, Poirier Y: Production of renewable polymers from crop plants. Plant J. 2008, 54: 684-701. 10.1111/j.1365-313X.2008.03431.x.
Budde CF, Riedel SL, Willis LB, Rha C, Sinskey AJ: Production of poly(3-hydroxybutyrate-co-3-hydroxyhexanoate) from plant oil by engineered Ralstonia eutropha strains. Appl Environ Microbiol. 2011, 77: 2847-2854. 10.1128/AEM.02429-10.
Fukui T, Suzuki M, Tsuge T, Nakamura S: Microbial synthesis of poly((R)-3-hydroxybutyrate-co-3-hydroxypropionate) from unrelated carbon sources by engineered Cupriavidus necator. Biomacromolecules. 2009, 10: 700-706. 10.1021/bm801391j.
Kawashima Y, Cheng W, Mifune J, Orita I, Nakamura S, Fukui T: Characterization and functional analyses of R-specific enoyl Coenzyme A hydratases in polyhydroxyalkanoate-producing Ralstonia eutropha. Appl Environ Microbiol. 2012, 78: 493-502. 10.1128/AEM.06937-11.
Matsusaki H, Abe H, Taguchi K, Fukui T, Doi Y: Biosynthesis of poly(3-hydroxybutyrate-co-3-hydroxyalkanoates) by recombinant bacteria expressing the PHA synthase gene phaC1 from Pseudomonas sp. 61–3. Appl Microbiol Biotechnol. 2000, 53: 401-409. 10.1007/s002530051633.
Mifune J, Nakamura S, Fukui T: Targeted engineering of Cupriavidus necator chromosome for biosynthesis of poly (3-hydroxybutyrate-co-3-hydroxyhexanoate) from vegetable oil. Can J Chem. 2008, 86: 621-627. 10.1139/v08-047.
Mifune J, Nakamura S, Fukui T: Engineering of pha operon on Cupriavidus necator chromosome for efficient biosynthesis of poly(3-hydroxybutyrate-co-3-hydroxyhexanoate) from vegetable oil. Polym Degrad Stab. 2010, 95: 1305-1312. 10.1016/j.polymdegradstab.2010.02.026.
Tsuge T, Yano K, Imazu S, Numata K, Kikkawa Y, Abe H, Taguchi S, Doi Y: Biosynthesis of polyhydroxyalkanoate (PHA) copolymer from fructose using wild-type and laboratory-evolved PHA synthases. Macromol Biosci. 2005, 5: 112-117. 10.1002/mabi.200400152.
Pohlmann A, Fricke WF, Reinecke F, Kusian B, Liesegang H, Cramm R, Eitinger T, Ewering C, Pötter M, Schwartz E, Strittmatter A, Voss I, Gottschalk G, Steinbüchel A, Friedrich B, Bowien B: Genome sequence of the bioplastic-producing “Knallgas” bacterium Ralstonia eutropha H16. Nat Biotechnol. 2006, 24: 1257-1262. 10.1038/nbt1244.
Peplinski K, Ehrenreich A, Döring C, Bömeke M, Reinecke F, Hutmacher C, Steinbüchel A: Genome-wide transcriptome analyses of the “Knallgas” bacterium Ralstonia eutropha H16 with regard to polyhydroxyalkanoate metabolism. Microbiology. 2010, 156: 2136-2152. 10.1099/mic.0.038380-0.
Brigham CJ, Budde CF, Holder JW, Zeng Q, Mahan AE, Rha C, Sinskey AJ: Elucidation of β-oxidation pathways in Ralstonia eutropha H16 by examination of global gene expression. J Bacteriol. 2010, 192: 5454-5464. 10.1128/JB.00493-10.
Marioni JC, Mason CE, Mane SM, Stephens M, Gilad Y: RNA-seq: an assessment of technical reproducibility and comparison with gene expression arrays. Genome Res. 2008, 18: 1509-1517. 10.1101/gr.079558.108.
Shendure J, Ji H: Next-generation DNA sequencing. Nat Biotechnol. 2008, 26: 1135-1145. 10.1038/nbt1486.
Pinto AC, Melo-Barbosa HP, Miyoshi A, Silva A, Azevedo V: Application of RNA-seq to reveal the transcript profile in bacteria. Genet Mol Res. 2011, 10: 1707-1718. 10.4238/vol10-3gmr1554.
Brigham CJ, Speth DR, Rha C, Sinskey AJ: Whole genome microarray and gene deletion studies reveal regulation of the polyhydroxyalkanoate production cycle by the stringent response in Ralstonia eutropha H16. Appl Environ Microbiol. 2012, 78: 8033-8044. 10.1128/AEM.01693-12.
Fukui T, Chou K, Harada K, Orita I, Nakayama Y, Bamba T, Nakamura S, Fukusaki E: Metabolite profiles of polyhydroxyalkanoate-producing Ralstonia eutropha H16. Metabolomics. 2013, doi: 10.1007/s11306-013-0567-0.
Fukui T, Doi Y: Efficient production of polyhydroxyalkanoates from plant oils by Alcaligenes eutrophus and its recombinant strain. Appl Microbiol Biotechnol. 1998, 49: 333-336. 10.1007/s002530051178.
Raberg M, Reinecke F, Reichelt R, Malkus U, König S, Pötter M, Fricke WF, Pohlmann A, Voigt B, Hecker M, Friedrich B, Bowien B, Steinbüchel A: Ralstonia eutropha H16 flagellation changes according to nutrient supply and state of poly(3-hydroxybutyrate) accumulation. Appl Environ Microbiol. 2008, 74: 4477-4490. 10.1128/AEM.00440-08.
Windhövel U, Bowien B: Identification of cfxR, an activator gene of autotrophic CO2 fixation in Alcaligenes eutrophus. Mol Microobiol. 1991, 5: 2695-2705. 10.1111/j.1365-2958.1991.tb01978.x.
Grzeszik C, Jeffke T, Schäferjohann J, Kusian B, Bowien B: Phosphoenolpyruvate is a signal metabolite in transcriptional control of the cbb CO2 fixation operons in Ralstonia eutropha. J Mol Microbiol Biotechnol. 2000, 2: 311-320.
Bowien B, Friedrich CG, Friedrich B: Formation of enzymes of autotrophic metabolism during heterotrophic growth of Alcaligenes eutrophus. J Gen Microbiol. 1981, 16: 69-78.
Kusian B, Bowien B: Organization and regulation of cbb CO2 assimilation genes in autotrophic bacteria. FEMS Microbiol Rev. 1997, 21: 135-155. 10.1111/j.1574-6976.1997.tb00348.x.
Raberg M, Bechmann J, Brandt U, Schlüter J, Uischner B, Voigt B, Hecker M, Steinbüchel A: Versatile metabolic adaptations of Ralstonia eutropha H16 to a loss of PdhL, the E3 component of the pyruvate dehydrogenase complex. Appl Environ Microbiol. 2011, 77: 2254-2263. 10.1128/AEM.02360-10.
Brämer CO, Steinbüchel A: The methylcitric acid pathway in Ralstonia eutropha: new genes identified involved in propionate metabolism. Microbiology. 2001, 147: 2203-2214.
Bruland N, Voss I, Brämer C, Steinbüchel A: Unravelling the C3/C4 carbon metabolism in Ralstonia eutropha H16. J Appl Microbiol. 2010, 109: 79-90.
Yoon SH, Han MJ, Lee SY, Jeong KJ, Yoo JS: Combined transcriptome and proteome analysis of Escherichia coli during high cell density culture. Biotechnol Bioeng. 2003, 81: 753-767. 10.1002/bit.10626.
Yang S, Tschaplinski TJ, Engle NL, Carroll SL, Martin SL, Davison BH, Palumbo AV, Rodriguez M, Brown SD: Transcriptomic and metabolomic profiling of Zymomonas mobilis during aerobic and anaerobic fermentations. BMC Genomics. 2009, 10: 34-49. 10.1186/1471-2164-10-34.
Kataoka M, Hashimoto K-I, Yoshida M, Nakamatsu T, Horinouchi S, Kawasaki H: Gene expression of Corynebacterium glutamicum in response to the conditions inducing glutamate overproduction. Lett Appl Microbiol. 2006, 42: 471-476. 10.1111/j.1472-765X.2006.01905.x.
Lawrence AG, Schoenheit J, He A, Tian J, Liu P, Stubbe J, Sinskey AJ: Transcriptional analysis of Ralstonia eutropha genes related to poly-(R)-3-hydroxybutyrate homeostasis during batch fermentation. Appl Microbiol Biotechnol. 2005, 68: 663-672. 10.1007/s00253-005-1969-3.
Lindenkamp N, Peplinski K, Volodina E, Ehrenreich A, Steinbüchel A: Impact of multiple β-ketothiolase deletion mutations in Ralstonia eutropha H16 on the composition of 3-mercaptopropionic acid-containing copolymers. Appl Environ Microbiol. 2010, 76: 5373-5382. 10.1128/AEM.01058-10.
Budde CF, Mahan AE, Lu J, Rha C, Sinskey AJ: Roles of multiple acetoacetyl coenzyme A reductases in polyhydroxybutyrate biosynthesis in Ralstonia eutropha H16. J Bacteriol. 2010, 192: 5319-5328. 10.1128/JB.00207-10.
Pötter M, Müller H, Steinbüchel A: Influence of homologous phasins (PhaP) on PHA accumulation and regulation of their expression by the transcriptional repressor PhaR in Ralstonia eutropha H16. Microbiology. 2005, 151: 825-833. 10.1099/mic.0.27613-0.
Pötter M, Müller H, Reinecke F, Wieczorek R, Fricke F, Bowien B, Friedrich B, Steinbüchel A: The complex structure of polyhydroxybutyrate (PHB) granules: four orthologous and paralogous phasins occur in Ralstonia eutropha. Microbiology. 2004, 150: 2301-2311. 10.1099/mic.0.26970-0.
Pfeiffer D, Jendrossek D: Interaction between poly(3-hydroxybutyrate) granule-associated proteins as revealed by two-hybrid analysis and identification of a new phasin in Ralstonia eutropha H16. Microbiology. 2011, 157: 2795-2807. 10.1099/mic.0.051508-0.
Pfeiffer D, Jendrossek D: Localization of PHB granule associated proteins during PHB granule formation and identification of two new phasins, PhaP6 and PhaP7, in Ralstonia eutropha H16. J Bacteriol. 2012, 194: 5909-5921. 10.1128/JB.00779-12.
Pfeiffer D, Wahl A, Jendrossek D: Identification of a multifunctional protein, PhaM, that determines number, surface to volume ratio, subcellular localization and distribution to daughter cells of poly(3-hydroxybutyrate), PHB, granules in Ralstonia eutropha H16. Mol Microobiol. 2011, 82: 936-951. 10.1111/j.1365-2958.2011.07869.x.
Kaddor C, Steinbüchel A: Effects of homologous phosphoenolpyruvate-carbohydrate phosphotransferase system proteins on carbohydrate uptake and poly(3-hydroxybutyrate) accumulation in Ralstonia eutropha H16. Appl Environ Microbiol. 2011, 77: 3582-3590. 10.1128/AEM.00218-11.
Michel H, Behr J, Harrenga A, Kannt A: Cytochrome c oxidase: structure and spectroscopy. Annu Rev Biophys Biomol Struct. 1998, 27: 329-356. 10.1146/annurev.biophys.27.1.329.
Kato M, Bao HJ, Kang C-K, Fukui T, Doi Y: Production of a novel copolyester of 3-hydroxybutyric acid and medium-chain-length 3-hydroxyalkanoic acids by Pseudomonas sp. 61–3 from sugars. Appl Microbiol Biotechnol. 1996, 45: 363-370. 10.1007/s002530050697.
Li H, Durbin R: Fast and accurate short read alignment with Burrows–Wheeler transform. Bioinformatics. 2009, 25: 1754-1760. 10.1093/bioinformatics/btp324.
Mortazavi A, Williams BA, McCue K, Schaeffer L, Wold B: Mapping and quantifying mammalian transcriptomes by RNA-Seq. Nat Methods. 2008, 5: 621-628. 10.1038/nmeth.1226.
Saeed AI, Sharov V, White J, Li J, Liang W, Bhagabati N, Braisted J, Klapa M, Currier T, Thiagarajan M, Sturn A, Snuffin M, Rezantsev A, Popov D, Ryltsov A, Kostukovich E, Borisovsky I, Liu Z, Vinsavich A, Trush V, Quackenbush J: TM4: a free, open-source system for microarray data management and analysis. Biotechniques. 2003, 34: 374-378.
Schäfer A, Tauch A, Jäger W, Kalinowski J, Thierbach G, Pühler A: Small mobilizable multi-purpose cloning vectors derived from the Escherichia coli plasmids pK18 and pK19: selection of defined deletions in the chromosome of Corynebacterium glutamicum. Gene. 1994, 145: 69-73. 10.1016/0378-1119(94)90324-7.
We thank Prof. K. Kurokawa (Department of Biological Information, Graduate School of Bioscience and Biotechnology, Tokyo Institute of Technology, Japan) for valuable assistance and suggestions for data analysis of RNA-seq. We also thank Assoc. Prof. T. Tsuge (Department of Innovative and engineered Materials, Interdisciplinary Graduate School of Science and Engineering, Tokyo Institute of Technology, Japan) for GC-MS analysis. This work was supported by MEXT Grant-in-Aid for Scientific Research on Priority Areas “Applied Genomics” (Grant Number 20018008) and that on Innovative Areas "Genome Science" (Grant Number 221S0002).
The authors declare that they have no competing interests.
RS carried out the experiments and data analyses, and wrote the manuscript. KC participated in the sample preparation and preliminary examination. YS carried out RNA-sequencing. IO and SN participated in the design and coordination of the study. TF designed the experiments and participated in the data processing and manuscript preparation. All authors read and approved the manuscript.