- Original article
- Open Access
Identification and characterization of levulinyl-CoA synthetase from Pseudomonas citronellolis, which differs phylogenetically from LvaE of Pseudomonas putida
AMB Expressvolume 9, Article number: 127 (2019)
Levulinic acid (LA) is a building block alternative to fermentable sugars derived from cellulosic biomass. Among LA catabolic processes in Pseudomonas putida KT2440, ligation of coenzyme A (CoA) to LA by levulinyl-CoA synthetase (LvaE) is known to be an initial enzymatic step in LA metabolism. To identify the genes involved in the first step of LA metabolism in Pseudomonas citronellolis LA18T, RNA-seq-based comparative transcriptome analysis was carried out for LA18T cells during growth on LA and pyruvic acid. The two most highly upregulated genes with LA exhibited amino acid sequence homologies to cation acetate symporter and 5-aminolevulinic acid dehydratase from Pseudomonas spp. Potential LA metabolic genes (lva genes) in LA18T that clustered with these two genes and were homologous to lva genes in KT2440 were identified, including lvaE2 of LA18T, which exhibited 35% identity with lvaE of KT2440. Using Escherichia coli cells with the pCold™ expression system, LvaE2 was produced and investigated for its activity toward LA. High performance liquid chromatography analysis confirmed that crude extracts of E. coli cells expressing the lvaE2 gene could convert LA to levulinyl-CoA in the presence of both HS-CoA and ATP. Phylogenetic analysis revealed that LvaE2 and LvaE formed a cluster with medium-chain fatty acid CoA synthetase, but they fell on different branches. Superimposition of LvaE2 and LvaE homology-based model structures suggested that LvaE2 had a larger tunnel for accepting fatty acid substrates than LvaE. These results indicate that LvaE2 is a novel levulinyl-CoA synthetase.
In recent years, much attention has been paid to the catalytic transformation of lignocellulose into key building block compounds under relatively mild conditions. An alternative building block to fermentable sugars is levulinic acid (LA), which is formed from cellulose or sugars in the presence of large quantities of mineral acids (Hayes et al. 2006; Pileidis and Titirici 2016) and is considered one of the top 12 building blocks by the US Department of Energy (Werpy and Petersen 2004). Although high concentrations of homogeneous acids such as H2SO4 and HCl have long been used for the synthesis of LA (Girisuta et al. 2008), heterogeneous acid catalysts have been applied recently to avoid the harsh and corrosive properties of mineral acids and the difficult recovery of such acids (Chen et al. 2011; Tominaga et al. 2011; Nemoto et al. 2015). At the industrial and commercial scale, LA is available for production of organic chemicals by companies such as GFBiochemicals, which operates a 2-kt per year production facility in Caserta, Italy (Pileidis and Titirici 2016). Among products from the conversion of LA into useful chemicals, levulinate esters, γ-valerolactone, and alkanes of various molecular weights can be used as fuels and fuel additives, while γ-valerolactone can be used in the production of valuable monomers (Bozell et al. 2000; Pileidis and Titirici 2016).
In addition to catalytic reactions that produce commodity and functional chemicals from LA, research into the production of value-added chemicals such as pharmaceuticals, cosmetics, and biopolymers through biotechnological processes is also important (Jaremko and Yu 2011; Berezina and Yada 2016; Habe et al. 2015a, b). However, incomplete understanding of the pathways and enzymes involved in LA metabolism by microorganisms has limited the potential of LA-based biorefinery applications based on biotechnological processes.
Recently, Rand et al. clarified a seven-gene operon that is essential for assimilating LA into the β-oxidation pathway in Pseudomonas putida KT2440 (Rand et al. 2017). This excellent study reported that lvaABCDE genes were upregulated in the presence of LA and were involved in the conversion of LA to an intermediate of the β-oxidation pathway, 3-hydroxyvaleryl-coenzyme A (3HV-CoA; Fig. 1). Purified LvaE, which is homologous to acyl-CoA synthetases with a putative CoA-binding region and an AMP-binding site, catalyzed the ligation of CoA to LA to yield levulinyl-CoA (LA-CoA). LvaD (oxidoreductase) catalyzed the reduction of LA-CoA to 4-hydroxyvaleryl-CoA (4HV-CoA) with NADH or NADPH. Both lvaA and lvaB, and especially the former, which is homologous to the kinase superfamily and phosphotransferase family of enzymes, were required for growth on LA, and these two enzymes may catalyze the conversion of 4HV-CoA to 4-phospho-valeryl-CoA (4PV-CoA). LvaC (putative oxidoreductase) may be involved in the conversion of 4PV-CoA to 3HV-CoA via pentanoyl-CoA. These results suggest a unique catabolic pathway for LA, especially in that the isomerization of 4HV-CoA to 3HV-CoA proceeds through a phosphorylated intermediate, 4PV-CoA (Zhang et al. 2009; Harris et al. 2011; Rand et al. 2017).
Among KT2440 mutants with disrupted lvaA, lvaB, lvaC, and lvaE genes, ΔlvaA, ΔlvaB, and ΔlvaC strains were unable to grow on LA, indicating that these three genes were essential for LA catabolism in P. putida. By contrast, ΔlvaE could grow on LA, suggesting that LA is also activated by other CoA synthetases in P. putida (Rand et al. 2017). Besides P. putida, homologues to lvaABCD can be found in a variety of Alpha-, Beta-, and Gammaproteobacteria, but lvaE homologues were not investigated due to the high promiscuity of acyl-CoA ligases (Rand et al. 2017). Purified LvaE exhibited enzymatic activity toward C4 to C6 carboxylic acids, but low activity toward shorter or longer carboxylic acids, suggesting enzymatic specificity for fatty acids of moderate chain length. No information is available regarding the involvement of other acyl-CoA ligase homologues, especially those showing low homology to LvaE (e.g., less than 40%). Further studies on the diversity of the initial enzymes used in LA catabolism will be important for elucidating LA catabolism.
In this study, we isolated several genes of Pseudomonas citronellolis LA18T (Habe et al. 2015a, 2017; Inaba et al. 2018) that were upregulated in the presence of LA by comparative transcriptomic analysis using RNA sequencing (RNA-seq). As a CoA-synthetase with relatively low homology to LvaE was found within the gene cluster, we investigated its activity toward LA, and its structural features were compared with those of LvaE through model building.
Materials and methods
All chemicals including LA were of the highest purity commercially available (98–100%; Sigma–Aldrich, Kanto Chemical, Wako Pure Chemical, Nacalai Tesque, Tokyo Chemical Industry). Levulinyl-CoA was synthesized by Tokyo Chemical Industry Co., Ltd. as a custom product.
Bacterial strains, media, and cultivation
An LA-utilizing bacterium, Pseudomonas citronellolis LA18T (JCM 33429; Habe et al. 2015a, 2017; Inaba et al. 2018), was routinely cultivated on Luria–Bertani (LB) broth (composition: 10 g L−1 tryptone, 5 g L−1 yeast extract, and 10 g L−1 NaCl). For comparative transcriptome analysis, LA medium C (composition: 20 g L−1 reagent LA, 2 g L−1 K2HPO4, 5 g L−1 (NH4)2SO4, 0.25 g L−1 MgSO4, and 5 g L−1 yeast extract; pH 6.5) was used. As a reference, LA medium C containing 20 g L−1 pyruvic acid instead of 20 g L−1 LA (PA medium C) was used. Strain LA18T was pre-cultivated for 1 day in 3 mL LB broth in a test tube. Seed cultures (0.5 mL) were transferred to a 300-mL Erlenmeyer flask containing 50 mL of LA medium C or PA medium C, and cultured for 4 days at 30 °C on a rotary shaker (150 rpm). Escherichia coli strains JM109 and DH5α were routinely cultivated at 37 °C using LB broth, as described by Sambrook and Russell (2001). If necessary, ampicillin (Ap) was added to the medium at a final concentration of 50 µg mL−1. Cell growth was evaluated based on optical density (OD) measurement at 600 nm.
RNA extraction and Illumina sequencing
Individual 2 mL samples of LA18T culture were collected on days 0, 2, and 3 during growth on LA (designated L0, L2, and L3, respectively) and on days 2 and 3 during growth on pyruvic acid (P2 and P3, respectively), for five samples in total. After centrifugation (15,300×g, 5 min, 4 °C), the resulting pellets were stored at − 80 °C until use. RNA was extracted from the pellets using the direct lysis protocol. Contaminating DNA was digested with DNase (RQ1 RNase-Free DNase, Promega, Fitchburg, WI, USA) and purified using the RNeasy Mini Kit (Qiagen, Venlo, Netherlands). The resultant total RNA was treated with a RiboMinus Transcriptome Isolation Kit for bacteria (Thermo Fisher Scientific, Waltham, MA, USA) to reduce rRNA levels, and then purified using an AMPure XP kit. Double-stranded cDNA libraries were prepared from the rRNA-depleted RNA samples using the NextUltraRNA library prep kit (New England Biolabs, Ipswich, MA, USA). Target-size cDNA (200–300 bp) was purified using the AMPure XP kit, followed by agarose gel electrophoresis. The size distribution and concentration of each purified cDNA sample was determined using a Bioanalyzer (Agilent 2100; Agilent Technologies, Santa Clara, CA, USA) and the Quant-iT PicoGreen dsDNA reagent and kit, respectively. An eight-picomolar cDNA sample was subjected to paired-end sequencing using a 300-cycle MiSeq reagent kit and MiSeq sequencer. RNA sequencing on the MiSeq platform provided 4,876,117 reads in total, corresponding to an average of 975,223 sequences per library (minimum, 699,410; maximum, 1,393,739).
Quality checking and expression level analysis of RNA sequences
Paired-end Illumina reads from each of the five samples were checked for quality using FastQC (Andrews, S. ; a quality control tool for high-throughput sequence data, available online at: http://www.bioinformatics.babraham.ac.uk/projects/fastqc). To ensure high sequence quality, the remaining sequencing adaptors, low-quality reads with a Phred score cutoff of 15 (leading and tailing sequences, Phred score > 20), and short reads of less than 100 bp were removed with the program Trimmomatic v0.30 using Illumina TruSeq 3 adapter sequences for adapter clipping (Bolger et al. 2014). Using genomic information for LA18T as a reference (DDBJ Sequence Read Archive accession codes BGPP01000001 and BGPP01000029; Inaba et al. 2018), paired-end RNA reads were mapped with the Bowtie2 program (Langmead and Salzberg 2012). After conversion of the output BAM files to BED files with the bamtobed program in BEDTools ver. 2.14.3 (Quinlan and Hall 2010), expression levels of the transcripts were evaluated by calculating transcripts per kilobase million (TPM) values using in-house scripts. The metatranscriptomic data obtained in this study have been deposited in the DDBJ Sequence Read Archive under accession code DRA007950.
Cloning and expression of the acyl-CoA synthetase-encoding gene (lvaE2) in E. coli
Total DNA preparation, plasmid isolation, and restriction enzyme digestion were performed as described previously (Sambrook and Russell 2001). The DNA Ligation Kit version 2 (Takara, Japan) and a QIAEXII Gel Extraction Kit (Qiagen) were used according to the manufacturers’ instructions. Other commercially available enzymes and kits were used as described by their manufacturers. Expression vectors for PCLA_07r0387 (designated lvaE2) were constructed as follows: 1596-bp and 1566-bp DNA fragments containing the putative lvaE2 gene were synthesized by Fasmac Co., Ltd., based on the LA18T genomic DNA sequence, to which NdeI and XbaI restriction sites were added at the 5′ and 3′ ends of the respective fragments. In the shorter DNA fragments (1566-bp), the 5′-terminal 30-bp region, corresponding to the N-terminal 10 amino acid sequence “MNFNLGIAAI”, was deleted from the longer DNA fragment, and the following methionine was used as a potential start codon for lvaE2. The longer and shorter DNA fragments were digested with two restriction enzymes then inserted into the corresponding sites in pCold™ IV DNA (Takara) to yield pCo7-387CoA-L and pCo7-387CoA-S, respectively.
Escherichia coli JM109 or DH5α cells carrying pCo7-387CoA-L or pCo7-387CoA-S were pre-cultivated in 5 mL of LB medium with Ap at 37 °C for 18 h, and the seed cultures (1.5 mL) were transferred to 300-mL Erlenmeyer flasks containing 30 mL of LB medium with Ap. The flasks were incubated on a rotary shaker (200 rpm) at 37 °C until the OD600 reached 0.8–1.0, and then immediately cooled at 15 °C for 30 min. Following the addition of 0 to 1.0 mM isopropyl-β-d-thiogalactopyranoside (IPTG), the flasks were further incubated for 20 h at 15 °C. Then, the cells were harvested through centrifugation, washed twice with 50 mM sodium phosphate buffer (pH 7), and resuspended in 5 mL of the same buffer. The cell suspensions were sonicated and centrifuged at 20,400×g at 4 °C for 60 min, and the resultant supernatants were stored at − 80 °C until use as crude cell extracts. The protein concentration of each crude extract was determined using a protein assay kit (Bio-Rad Laboratories, Hercules, CA, USA). The production of LvaE2 was confirmed through SDS-PAGE with a 12.5% polyacrylamide gel. The gels were stained for protein detection with Coomassie Brilliant Blue Stain Solutions A and B (Nacalai Tesque).
In vitro bioconversion of LA to levulinyl-CoA using crude enzymes
The enzymatic conversion of LA to LA-CoA with crude cell extracts containing LvaE2 was investigated by determining the time-dependent increase in the high-performance liquid chromatography (HPLC) peaks of LA-CoA. The reaction mixture (1500 μL total), which contained 50 mM sodium phosphate buffer (pH 7), 20 mM sodium levulinate (60 μL of 500 mM stock solution), 10 mM coenzyme A (HS-CoA; 15 μL of 1 M stock solution), 5 mM ATP (7.5 μL of 1 M stock solution), and approximately 300 μL of crude cell extract of E. coli JM109 or DH5α carrying pCo7-387CoA-L (0.4 μg mL−1), was incubated at 30 °C for 0 to 20 h. Samples for HPLC analysis were harvested at 0, 15, 30, 60, and 120 min and 20 h after beginning the incubation. As control experiments, reaction mixtures without HS-CoA or ATP were also tested. In addition, crude extracts of E. coli JM109 or DH5α cells carrying pCold™ IV DNA or pCo7-387CoA-S were used for comparison.
After centrifugation of the reaction mixtures, the supernatants were analyzed using HPLC with an LC-20AD HPLC pump (1.0 mL min−1 flow rate) and an SPD-20AV detector (Shimadzu) equipped with a TSK-GEL ODS-100 V column (150 × 4.6 mm, TOSOH)] to detect the peak from levulinyl-CoA. A mobile phase of 150 mM NaH2PO4 with 15% (v/v) methanol was used with this column. During analysis, the column temperature was maintained at 40 °C. The retention time of the reaction product was compared with that of synthesized LA-CoA. Co-chromatography experiments involving a mixed sample of the reaction product and synthesized LA-CoA were also performed.
Phylogenetic tree construction and molecular model building
Multiple alignments were constructed with CLUSTAL W and phylogenetic analyses based on the neighbor-joining method were performed using MEGA7 software (Kumar et al. 2016). Molecular model building for LvaE2 from LA18T and LvaE from KT2440 was performed with an automated mode of SWISS-MODEL server (https://swissmodel.expasy.org/) using 1ult.1.A and 3r44.1 A as templates, respectively.
Briefly, suitable templates for the modeling analysis were identified based on BLAST and HHblits analyses of the amino acid sequences of the query proteins. Then, the templates showing high similarities scores were sorted according to the expected quality of the resulting models, as estimated primarily by Global Model Quality Estimation (GMQE) scores (For details, see the introduction of SWISS-MODEL: https://swissmodel.expasy.org/docs/help). Resultantly, top-ranked templates, i.e., 1ult.1.A and 3r44.1 A, were used for the 3D modeling. Structural analysis of the LvaE2 and LvaE models was performed using the PyMOL Molecular Graphics System (Version 1.4.1; Schrödinger, LLC).
Comparative transcriptome analysis
Identification of genes involved in LA catabolism was carried out using a comparative RNA-seq technique with the transcriptomes of P. citronellolis LA18T grown on LA and pyruvic acid (Additional file 1: Figure S1). Comparative transcriptome analysis revealed some upregulated genes when LA18T cells were cultivated with LA. In LA18T cells, 571 genes in sample L3 were found to be upregulated by at least 2.0-fold compared with the P2 sample (L3/P2 ratio); the ten most upregulated genes are listed in Table 1. The two most strongly upregulated genes (PCLA_07r0385 and PCLA_07f0384) were located adjacent to each other in the genome and showed amino acid sequence homology with cation acetate symporters from P. citronellolis (99% identity) and P. pseudoalcaligenes (85% identity) and with 5-aminolevulinic acid dehydratases (ALADs; porphobilinogen synthase) from P. citronellolis (100% identity) and P. putida (93% identity), respectively.
Analysis of gene clusters containing genes upregulated in the presence of LA
To identify the open reading frames (ORFs) flanking the two most strongly upregulated genes, a genomic locus of approximately 11.1 kb containing PCLA_07r0385 and PCLA_07f0384 was re-analyzed in this study (PCLA_07f00384 to PCLA_07f0396; Fig. 2 and Table 2). The nucleotide sequence was deposited in the DDBJ, EMLB, and GenBank nucleotide sequence databases under accession number LC458675.
PCLA_07f0384: ALAD. The deduced amino acid sequences shared the most homology with ALAD, which catalyzes the asymmetric condensation and cyclization of two 5-aminolevulinate molecules, the first common step in the biosynthesis of tetrapyrrole pigments such as porphyrin, chlorophyll, vitamin B12, siroheme, phycobilin, and cofactor F430 (Table 2). The product of PCLA_07f0384 contains a highly conserved metal-binding site for Zn2+, D-X-C-X-C-X-(Y/F)-X3-G-(H/Q)-C-G, but not an alternative cysteine-free site for Mg2+, D-X-A-L-D-X-(F/Y)-X3-G-(H/Q)-D-G (Jaffe 2016), suggesting an absolute Zn2+ requirement for the enzyme (data not shown).
PCLA_07r0385 to 07r0389: putative LA-assimilating gene cluster 1 (transporter and CoA ligase). We found a gene cluster of three ORFs encoding homologues of the acetate symporter ActP (PCLA_07r0385), fatty acid-CoA ligase (PCLA_07r0387), and regulatory protein (PCLA_07r0389) in the same direction of transcription. The polypeptide encoded by PCLA_07r0385, 07r0387, and 07r0389 showed 64%, 35%, and 52% identity, respectively, with LvaG, LvaE, and LvaR from P. putida KT2440 (Table 2). In addition, within the cluster, ORF PCLA_07r0386 (a homologue of a DUF485 domain-containing protein homologue; 72 amino acids) encoded a product with 35 to 39% identity with a hypothetical protein that clustered with the putative membrane protein ActP and inner membrane protein YjcH from E. coli. This protein is likely involved in organic acid transport along with PCLA_07r0385, as suggested for LvaF from P. putida (Rand et al. 2017).
PCLA_07f0390 to 07f0396: putative LA-assimilating gene cluster 2 (conversion of LA-CoA to 3HV-CoA). Four ORFs encoding possible LA-assimilating genes were located adjacent to the gene cluster of PCLA_07r0385 to 07r0389. The deduced amino acid sequence of PCLA_07f0390 shared 59% identity with the phosphotransferase family protein LvaA from P. putida KT2440. By contrast, the polypeptide encoded by PCLA_07f0393 showed 99% identity with a histidine phosphatase family protein from P. citronellolis. The deduced amino acid sequences of PCLA_07f0394 and 07f0396 showed 78% and 67% identities with the acyl-CoA dehydrogenase LvaC and short-chain dehydrogenase reductase LvaD, respectively, from P. putida KT2440.
Expression of lvaE2 (PCLA_07r0387) in E. coli cells
The gene PCLA_07r0387, encoding the fatty acid-CoA ligase homologue, was designated lvaE2. Expression vectors containing lvaE2 were first constructed using the pET-26b(+) backbone with 6× His N-terminal fusion using the pET expression system with E. coli BL21 (DE3) cells. However, a band with a molecular mass of 59 kDa was observed in the precipitates but not in the supernatants. The same result was observed using the same expression system without His-tag fusion, i.e., native LvaE2 (data not shown).
Expression vectors containing lvaE2 were then constructed using the pCold™ IV backbone, and IPTG-induced E. coli JM109 or DH5α cells carrying pCo7-387CoA-L were cultivated for the production of LvaE2. In both strains, JM109 and DH5α, the band at 59 kDa corresponding to LvaE2 was confirmed through SDS-PAGE from the supernatants as well as the precipitates (Additional file 1: Figure S2). By contrast, bands at 59 kDa were not observed in crude cell extracts of E. coli JM109 or DH5α cells containing not only the pCold™ IV vector (Additional file 1: Figure S1), but also pCo7-387CoA-S (data not shown).
In vitro bioconversion of LA to levulinyl-CoA using crude enzymes
To investigate the levulinyl-CoA synthase activity of LvaE2, we monitored time-dependent LA-CoA production from LA by measuring the increase of HPLC peaks for LA-CoA. Using cell-free extracts of E. coli JM109 or DH5α expressing lvaE2, enzymatic activity was determined in the presence of sodium levulinate, HS-CoA, and ATP (Fig. 3). The HPLC peak area for LA-CoA (retention time: 13.6 min) increased from 0 min to 20 h, along with a decrease in the peak for HS-CoA (retention time: 4.3 min), whereas no peak for LA-CoA was observed in cell-free extracts of E. coli JM109 or DH5α cells carrying the pCold™ IV vector (control) or pCo7-387CoA-S. In addition, no peak for LA-CoA was detected in HPLC analyses when ATP or HS-CoA was excluded from the reaction mixture. The reaction also did not proceed with any samples from resuspended precipitates. These results indicate that LvaE2 (PCLA_07r0387 product) has enzymatic activity toward LA, and therefore acts as an LA-CoA synthase (LA-CoA ligase).
Molecular modeling of LvaE2 from LA18T and LvaE from KT2440
Structural comparison was carried out through homology modeling of LvaE2 from LA18T and LvaE from KT2440. The two models have features similar to acyl-CoA synthetase from Thermus thermophilus (e.g., Hisanaga et al. 2004), including a small and globular C-terminal domain (Fig. 4a (LvaE2), b (LvaE), and d (superimposition), lower left part of the structure), a large and globular N-terminal domain (Fig. 4a, b, upper right part of the structure), and an active site located between these domains (yellow in Fig. 4a–c). Superimposition of the molecular surfaces of LvaE2 (black) and LvaE (magenta) revealed a predicted loop region in the C-terminal domain of the LvaE model, which is located in a tunnel region of LvaE2, as indicated by the red arrow in Fig. 4e. Although the overall structures of the C-terminal domains of the two models were relatively similar, the structures of the linker region between the C- and N-terminal domains (blue arrow in Fig. 4e, f) differed, resulting in a difference in the rotation angle of the C-terminal domains against the N-terminal domains. In LvaE, three amino acid residues (Ala437, Lys438, and Asp439) in the linker region form a short α-helix structure, whereas the equivalent three amino acid residues in LvaE2 (Arg428, Ile429, and Lys430) may form a loop structure (Fig. 4f).
The present study was undertaken to identify the genes involved in LA assimilation by P. citronellolis LA18T through RNA-seq-based comparative transcriptome analysis. The comparison of LA- and PA-grown LA18T cells allowed identification of the two most strongly upregulated genes (PCLA_07r0385 and PCLA_07f0384), which were highly homologous to cation acetate symporter and ALAD, respectively (Table 1). These two genes were located adjacent to each other, but with different transcriptional directions (Fig. 2).
In the DNA region containing PCLA_07r0385 and PCLA_07f0384, several other genes homologous to lva operon genes of KT2440 were identified (Fig. 2). In addition to an lvaR homologue (52% identity at the amino acid level; putative transcriptional regulator for LA assimilation), an LvaA homologue (59% identity) associated with the kinase superfamily and phosphotransferase family of enzymes was also observed (Fig. 2). In KT2440, LvaB, a hypothetical protein only 12 kDa in size, was demonstrated to interact with LvaA through a pulldown experiment, and both proteins LvaA and LvaB catalyzed the conversion of 4HV-CoA to 4PV-CoA (Rand et al. 2017). By contrast, in LA18T, no gene homologous to lvaB was found in the DNA region analyzed, but a gene homologous to histidine phosphatase family proteins was found adjacent to the lvaA homologue (PCLA_07f0393). This protein may be involved in the removal of a phosphate group from 4-PV-CoA in LA18T, although LvaC in KT2440 may be responsible for both phosphate group removal from 4-PV-CoA to produce enoyl-CoA and the subsequent hydration reaction producing 3-HV-CoA (Rand et al. 2017). In addition, the LvaC homologue in LA18T may participate in the reaction. Functional analysis of the histidine phosphatase homologue is necessary to clarify the difference between the mechanisms for transforming 4-PV-CoA into 3-HV-CoA in KT2440 and LA18T.
Among lva gene homologues in LA18T (Fig. 2), we demonstrated that the fatty acid-CoA ligase homologue, LvaE2, could catalyze the transformation of LA into LA-CoA through in vitro bioconversion experiments using crude enzymes from recombinant E. coli. In contrast to LvaE in KT2440, LvaE2 could not be produced in the soluble fraction using E. coli BL21 (DE3) cells with the pET expression system, although various cultivation conditions (e.g., IPTG concentration, temperature, and with or without the His-tag) were tested. The N-terminal His-tagged LvaE from KT2440 was successfully purified and investigated for its activity towards short- and medium-chain fatty acids, showing activity on C4–C6 carboxylic acids including LA and 4-hydroxyvaleric acid (Rand et al. 2017). In the CoA ligase activity assay, the amount of pyrophosphate released during the CoA ligase reaction was measured (absorbance at 360 nm). For this method, enzyme purification is needed because crude extracts contain some pyrophosphate and CoA ligases other than LvaE. By contrast, when investigating substrate specificity of LvaE2 in our bioconversion experiments, CoA derivatives of various carboxylic acids are needed as pure compounds for HPLC analysis, most of which are not commercially available. Although LvaE2 was hardly produced in the soluble fraction using E. coli cells with the pCold™ IV DNA system, increasing LvaE2 production through the use of other expression systems should be investigated for isolation of the enzyme.
Fatty acyl-CoA synthetases, required for conversion of long-chain fatty acids to their CoA thioesters, are defined based on the length of the aliphatic chain of their substrates as short-, medium-, and long-chain fatty acid CoA synthetases (Hisanaga et al. 2004). Enzymes in these classes use C2–C4, C4–C12, and C12–C22 fatty acids, respectively, as substrates. The functional role of the long-chain fatty acid CoA synthetase FadD from E. coli has been intensively studied, suggesting cooperative activity between FadD and FadL, the latter of which is an outer membrane fatty acid transport protein, that essentially renders the process of fatty acid transport unidirectional (Weimar et al. 2002). FadD activity was detected not only within the membrane but also in soluble fractions, suggesting that FadD moves between the bacterial cytosol and inner membrane to promote vectorial esterification of exogenous fatty acids (Mangroo and Gerber 1993). In addition, FadD was thought to be peripherally associated with the bacterial inner membrane (Mangroo and Gerber 1993). By contrast, LvaE from KT2440 is apparently classified as a medium-chain fatty acid CoA synthetase due to its utilization of C4–C6 carboxylic acids (Rand et al. 2017), and the recruitment process that brings medium-chain fatty acid CoA synthetases to the inner membrane remains unknown. The cooperative activity of LvaE and outer membrane proteins such as LvaG still remains to be investigated. Phylogenetic analysis revealed that LvaE2 from LA18T did not cluster with the long-chain fatty acid CoA synthetase FadD, but rather formed a cluster with the medium-chain fatty acid CoA synthetase LvaE. However, LvaE2 was not located on the same branch as LvaE and FadK (Additional file 1: Figure S3). The phylogenetic relationships among LvaE2, LvaE, and FadD suggest that LvaE2 may belong to medium-chain fatty acid CoA synthetases, but is phylogenetically distinct from LvaE in KT2440.
To clarify the differences between LvaE2 from LA18T and LvaE from KT2440, homology models of the two enzymes were compared. The overall structures of both the C- and N-terminal domains of the two models were relatively similar, whereas the structures of the linker region between the terminal domains (blue arrow in Fig. 4e, f) differed, causing a difference in the rotation angle of the C-terminal domains against the N-terminal domains. According to analysis of the structure of Thermus thermophilus acyl-CoA synthetase co-crystalized with myristoyl-AMP (Hisanaga et al. 2004), the length of the tunnel is hypothesized to determine substrate specificity, because myristoyl-AMP rests in the tunnel, which is well suited to accommodating its long hydrophobic tail. A similar mechanism has been proposed for the medium-chain specificity of the human homolog (Kochan et al. 2009). Considering these facts, the relatively rigid structure of the α-helix in the linker region of LvaE may determine the size of the tunnel region and cause strict substrate specificity for C4 to C6 fatty acids. Compared to LvaE, which has a predicted loop region at the entrance of the tunnel, no such loop region was located in the tunnel of LvaE2 (red arrow in Fig. 4e), suggesting that LvaE2 may exhibit substrate specificity toward fatty acids longer than those of LvaE. To investigate this prediction, a method for more efficient expression and purification of LvaE2 should be developed, but the structural differences between LvaE2 and LvaE may make it difficult to produce LvaE2 using E. coli.
In summary, a gene cluster that may be involved in LA catabolism was obtained from P. citronellolis LA18T using a comparative RNA-seq technique with LA18T cells grown on LA and pyruvic acid, providing the second example of LA catabolic genes following those of P. putida KT2440 (Rand et al. 2017). Among the genes identified, the initial enzyme for LA catabolism, levulinyl-CoA synthase LvaE2, which differs phylogenetically from LvaE in KT2440, was produced in E. coli cells and was confirmed to have activity toward LA. Among the genes encoding subsequent enzymatic steps, some differences were found between LA18T and KT2440 lva gene clusters; in particular, LvaB is not found within the gene cluster in LA18T, and instead, a gene encoding a phosphatase-family protein is located in the cluster. Further functional analysis studies of LA18T lva genes are necessary to elucidate the detailed mechanisms of LA metabolism.
Availability of data and materials
Pseudomonas citronellolis LA18T has been deposited in RIKEN BRC under accession number JCM 33429. The nucleotide sequence was deposited in the DDBJ, EMLB, and GenBank nucleotide sequence databases under accession number LC458675.
Berezina N, Yada B (2016) Improvement of the poly(3-hydroxybutyrate-co-3-hydroxyvalerate) (PHBV) production by dual feeding with levulinic acid and sodium propionate in Cupriavidus necator. N Biotechnol 33:231–236. https://doi.org/10.1016/j.nbt.2015.06.002
Bolger AM, Lohse M, Usadel B (2014) Trimmomatic: a flexible trimmer for Illumina sequence data. Bioinformatics 30:2114–2120. https://doi.org/10.1093/bioinformatics/btu170
Bozell JJ, Moens L, Elliott DC, Wang Y, Neuenscwander GG, Fitzpatrick SW, Bilski RJ, Jarnefeld JL (2000) Production of levulinic acid and use as a platform chemical for derived products. Resour Conserv Recycl 28:227–239. https://doi.org/10.1016/S0921-3449(99)00047-6
Chen H, Yu B, Jin S (2011) Production of levulinic acid from steam exploded rice straw via solid superacid, S2O8 2−/ZrO2-SiO2-Sm2O3. Bioresour Technol 102:3568–3570. https://doi.org/10.1016/j.biortech.2010.10.018
Girisuta B, Danon B, Manurung R, Janssen LPBM, Heeres HJ (2008) Experimental and kinetic modelling studies on the acid-catalysed hydrolysis of the water hyacinth plant to levulinic acid. Bioresour Technol 99:8367–8375. https://doi.org/10.1016/j.biortech.2008.02.045
Habe H, Sato S, Morita T, Fukuoka T, Kirimura K, Kitamoto D (2015a) Bacterial production of short-chain organic acids and trehalose from levulinic acid: a potential cellulose-derived building block as a feedstock for microbial production. Bioresour Technol 177:381–386. https://doi.org/10.1016/j.biortech.2014.11.048
Habe H, Sato S, Morita T, Fukuoka T, Kirimura K, Kitamoto D (2015b) Isolation and characterization of bacterial strains with the ability to utilize high concentrations of levulinic acid, a platform chemical from inedible biomass. Biosci Biotechnol Biochem 79:1552–1555. https://doi.org/10.1080/09168451.2015.1031076
Habe H, Kondo S, Sato Y, Hori T, Kanno M, Kimura N, Koike H, Kirimura K (2017) Electrodialytic separation of levulinic acid catalytically synthesized from woody biomass for use in microbial conversion. Biotechnol Prog 33:448–453. https://doi.org/10.1002/btpr.2425
Harris SR, Zhang G-F, Sadhukhan S, Murphy AM, Tomcik KA, Vazquez EJ, Anderson VE, Tochtrop GP, Brunengraber H (2011) Metabolism of levulinate in perfused rat livers and live rats: conversion to the drug of abuse 4-hydroxypentanoate. J Biol Chem 286:5895–5904. https://doi.org/10.1074/jbc.M110.196808
Hayes DJ, Fitzpatrick S, Hayes MHB, Ross JRH (2006) The biofine process—Production of levulinic acid, furfral, and formic acid from lignocellulosic feedstocks. In: Kamm B, Gruber PR, Kamm M (eds) Biorefineries—industrial processes and products, vol 1. Wiley-VCH Verlag GmbH & Co. KGaA, Weinheim, pp 139–164
Hisanaga Y, Ago H, Nakagawa N, Hamada K, Ida K, Yamamoto M, Hori T, Arii Y, Sugahara M, Kuramitsu S, Yokoyama S, Miyano M (2004) Structural basis of the substrate-specific two-step catalysis of long chain fatty acyl-CoA synthetase dimer. J Biol Chem 279:31717–31726. https://doi.org/10.1074/jbc.M400100200
Inaba T, Sato Y, Koike H, Hori T, Kanno M, Kimura N, Kirimura K, Habe H (2018) Draft genome sequence of Pseudomonas citronelollis LA18T, a bacterium that use levulinic acid. Microbiol Resour Announc 7(5):e00906-18. https://doi.org/10.1128/MRA.00906-18
Jaffe EK (2016) The remarkable character of porphobilinogen synthase. Acc Chem Res 49:2509–2517. https://doi.org/10.1021/acs.accounts.6b00414
Jaremko M, Yu J (2011) The initial metabolic conversion of levulinic acid in Cupriavidus necator. J Biotechnol 155:293–298. https://doi.org/10.1016/j.jbiotec.2011.07.027
Kochan G, Pilka ES, von Delft F, Oppermann U, Yue WW (2009) Structural snapshots for the conformation-dependent catalysis by human medium-chain acyl-coenzyme A synthetase ACSM2A. J Mol Biol 388:997–1008. https://doi.org/10.1016/j.jmb.2009.03.064
Kumar S, Stecher G, Tamura K (2016) MEGA7: molecular evolutionary genetics analysis version 7.0 for bigger datasets. Mol Biol Evol 33:1870–1874. https://doi.org/10.1093/molbev/msw054
Langmead B, Salzberg SL (2012) Fast gapped-read alignment with Bowtie 2. Nat Methods 9:357–359. https://doi.org/10.1038/nmeth.1923
Mangroo D, Gerber GE (1993) Fatty acid uptake in Escherichia coli: regulation by recruitment of fatty acyl-CoA synthetase to the plasma membrane. Biochem Cell Biol 71:51–56. https://doi.org/10.1139/o93-008
Nemoto K, Tominaga K, Sato K (2015) Facile and efficient transformation of lignocelluloses into levulinic acid using an AlCl3·6H2O/H3PO4 hybrid acid catalyst. Bull Chem Soc Jpn 88:1752–1754. https://doi.org/10.1246/bcsj.20150266
Pileidis FD, Titirici MM (2016) Levulinic acid biorefineries: new challenges for efficient utilization of biomass. Chemsuschem 9:562–582. https://doi.org/10.1002/cssc.201501405
Quinlan AR, Hall IM (2010) BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics 26:841–842. https://doi.org/10.1093/bioinformatics/btq033
Rand JM, Pisithkul T, Clark RL, Thiede JM, Mehrer CR, Agnew DE, Campbell CE, Markley AL, Price MN, Ray J, Wetmore KM, Suh Y, Arkin AP, Deutschbauer AM, Amador-Noguez D, Pfleger BF (2017) A metabolic pathway for catabolizing levulinic acid in bacteria. Nat Microbiol 2:1624–1634. https://doi.org/10.1038/s41564-017-0028-z
Sambrook J, Russell DW (2001) Molecular cloning, a laboratory manual, 3rd edn. Cold Spring Harbor, Cold Spring Harbor Laboratory
Tominaga K, Mori A, Fukushima Y, Shimada S, Sato K (2011) Mixed-acid systems for the catalytic synthesis of methyl levulinate from cellulose. Green Chem 13:810–812. https://doi.org/10.1074/jbc.M107022200
Weimar JD, DiRusso CC, Delio R, Black PN (2002) Functional role of fatty acyl-coenzyme A synthetase in the transmembrane movement and activation of exogenous long-chain fatty acids. J Biol Chem 277:29369–29376. https://doi.org/10.1074/jbc.M107022200
Werpy T, Petersen G (2004) Top value added chemicals from biomass. Department of Energy, Washington DC, pp 45–48
Zhang G-F, Kombu RS, Kasumov T, Han Y, Sadhukhan S, Zhang J, Sayre LM, Ray D, Gibson KM, Anderson VA, Tochtrop GP, Brunengraber H (2009) Catabolism of 4-hydroxyacids and 4-hydroxynonenal via 4-hydroxy-4-phosphoacyl-CoAs. J Biol Chem 284:33521–33534. https://doi.org/10.1074/jbc.M109.055665
The authors thank Susumu Kondo, Mariko Kamata, and Shohei Kawamoto for technical support.
This work was partly supported by the Institute for Fermentation, Osaka.
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