JB
Home Help [Feedback] [For Subscribers] [Archive] [Search] [Contents]
This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Services
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrow Copyright Information
Right arrow Books from ASM Press
Right arrow MicrobeWorld
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Sakai, Y.
Right arrow Articles by Kato, N.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Sakai, Y.
Right arrow Articles by Kato, N.
Journal of Bacteriology, November 2004, p. 7214-7220, Vol. 186, No. 21
0021-9193/04/$08.00+0     DOI: 10.1128/JB.186.21.7214-7220.2004
Copyright © 2004, American Society for Microbiology. All Rights Reserved.

Role of {alpha}-Methylacyl Coenzyme A Racemase in the Degradation of Methyl-Branched Alkanes by Mycobacterium sp. Strain P101

Yasuyoshi Sakai,1 Hironori Takahashi,1 Yuori Wakasa,1 Tetsuya Kotani,1 Hiroya Yurimoto,1 Nobuya Miyachi,2 Paul P. Van Veldhoven,3 and Nobuo Kato1*

Division of Applied Life Sciences, Graduate School of Agriculture, Kyoto University, Kitashirakawa Sakyo-ku, Kyoto,1 New Products & Technology Lab, COSMO Research Institute, Satte, Saitama, Japan,2 Katholieke Universiteit Leuven, Campus Gasthuisberg, Department Moleculaire Celbiologie, Afdeling Farmakologie, Leuven, Belgium3

Received 30 June 2004/ Accepted 1 August 2004


   ABSTRACT
Top
 Abstract
Introduction
 Materials and Methods
 Results
 Discussion
 References
 
A new isolate, Mycobacterium sp. strain P101, is capable of growth on methyl-branched alkanes (pristane, phytane, and squalane). Among ca. 10,000 Tn5-derived mutants, we characterized 2 mutants defective in growth on pristane or n-hexadecane. A single copy of Tn5 was found to be inserted into the coding region of mcr ({alpha}-methylacyl coenzyme A [{alpha}-methylacyl-CoA] racemase gene) in mutant P1 and into the coding region of mls (malate synthase gene) in mutant H1. Mutant P1 could not grow on methyl-branched alkanes. The recombinant Mcr produced in Escherichia coli was confirmed to catalyze racemization of (R)-2-methylpentadecanoyl-CoA, with a specific activity of 0.21 µmol · min–1 · mg of protein–1. Real-time quantitative reverse transcriptase PCR analyses indicated that mcr gene expression was enhanced by the methyl-branched alkanes pristane and squalane. Mutant P1 used (S)-2-methylbutyric acid for growth but did not use the racemic compound, and growth on n-hexadecane was not inhibited by pristane. These results suggested that the oxidation of the methyl-branched alkanoic acid is inhibited by the (R) isomer, although the (R) isomer was not toxic during growth on n-hexadecane. Based on these results, Mcr is suggested to play a critical role in ß-oxidation of methyl-branched alkanes in Mycobacterium. On the other hand, mutant H1 could not grow on n-hexadecane, but it partially retained the ability to grow on pristane. The reduced growth of mutant H1 on pristane suggests that propionyl-CoA is available for cell propagation through the 2-methyl citric acid cycle, since propionyl-CoA is produced through ß-oxidation of pristane.


   INTRODUCTION
Top
 Abstract
 Introduction
Materials and Methods
 Results
 Discussion
 References
 
Highly branched isoprenoid alkanes, such as pristane (2,6,10,14-tetramethylpentadecane), phytane (3,7,11,15-tetramethylhexadecane), and squalane (2,6,10,15,19,23-hexamethyltetracosane), normally occur in crude oil (3). Among the branched alkanes, the biodegradation of pristane has been most extensively studied. The oxidation pathway of pristane has been established based on analyses of the metabolic intermediates formed from pristine by using different gram-positive bacteria, such as Brevibacterium sp. (26), Corynebacterium sp. (22), Rhodococcus sp. (23), Nocardia globerula 432 (1), and Mycobacterium fortuitum (8). The combination of the findings suggests that pristane is oxidized to pristanic acid and then esterified with coenzyme A (CoA) to form pristanoyl-CoA, which is ß-oxidized. In six successive cycles of ß-oxidation, propionyl-CoA and acetyl-CoA are alternately released (26).

The degradation of methyl-branched chain fatty acids has also been investigated in mammalian cells (38). The methyl-branched fatty acids phytanic acid (3,7,11,15-tetramethylhexadecanoic acid) and pristanic acid (2, 6,10,14-tetramethylpentadecanoic acid) are present in the human diet. Phytanic acid is derived from chlorophyll-bound phytol and is converted to pristanic acid by {alpha}-oxidation in the peroxisomes. The CoA thioester pristanoyl-CoA is further ß-oxidized, first by two to three cycles in the peroxisomes and then later by cycles in the mitochondria (11, 18, 36).

The methyl groups of pristanic acid that are formed by {alpha}-oxidation or are present in the human diet are in the (R) configuration at positions 6 and 10 (21), while the methyl group of carbon 2 occurs in both the (R) and (S) configurations (28, 37). Because only the CoA ester with the 2-methyl group in the (S) configuration can be degraded by mammalian ß-oxidation, (2R)-pristanoyl-CoA needs to be converted to the (2S) stereoisomer (27, 28, 35), a reaction catalyzed by {alpha}-methylacyl-CoA racemase (2, 11).

The stereochemistry of bacterial pristane oxidation seems to be more complicated than that of mammalian pristanic acid oxidation. Some bacteria are capable of degrading the pristane present in crude oil, which is a mixture of a variety of stereoisomers at C-6 and C-10. Pristane is a common constituent of the lipids of many marine organisms (9), and a typical biogenic pristane, which is obtained from shark liver, has a (6R,10S)-meso configuration (9). In contrast, pristane of fossil origin is a mixture of diastereomers. M. fortuitum is known to use several configurations of pristane and preferentially oxidizes the biogenic (6R,10S) isomer. However, previous reports (4, 8, 9) have not been concerned with the stereospecificity of ß-oxidation, and both enzymological information and genetic information on bacterial pristanic acid oxidation are very limited. Recently, Bhaumik et al. found three genes, mcr, far, and Rv3727, which encode proteins homologous to mammalian {alpha}-methylacyl-CoA racemase in the Mycobacterium tuberculosis genome (5). Also, a putative {alpha}-methylacyl-CoA racemase gene was found in a gene cluster for isoprene metabolism in Rhodococcus sp. strain AD45 (34).

Similar to n-alkane oxidation, methyl-branched alkanes are first oxidized to the corresponding carboxylic acids and then oxidized through ß-oxidation. The most unusual feature of methyl-branched alkane oxidation is that the oxidized intermediates of methyl-branched alkanes are mixtures of stereoisomers. Thus, the stereospecificities of the reactions should be examined in order to understand the microbial degradation of methyl-branched alkanes. In this study, we isolated a new organism, Mycobacterium sp. strain P101, which is able to use several methyl-branched alkanes, including pristane, phytane, and squalane, as well as a variety of n-alkanes. After Tn5 mutagenesis, we isolated two mutants that were defective for growth on pristane and n-hexadecane, and the disrupted genes encoded {alpha}-methylacyl-CoA racemase and malate synthase, respectively. Judging from the growth characteristics of the mutants, we suggest that {alpha}-methylacyl-CoA racemase is essential for the oxidation of methyl-branched alkanes. This paper is the first report confirming the physiological role of {alpha}-methylacyl-CoA racemase in prokaryotes and also provides evidence for stereochemical control during bacterial ß-oxidation of methyl-branched fatty acids.


   MATERIALS AND METHODS
Top
 Abstract
 Introduction
 Materials and Methods
Results
 Discussion
 References
 
Enrichment and isolation of a pristane-grown bacterium. A pristane-utilizing bacterium was isolated from a soil sample after several cycles of enrichment culturing under aerobic conditions in NA medium containing 0.5% pristane (Tokyo Kasei, Tokyo Japan). NA medium contained (per liter) 3.2 g of Na2HPO4 · 12H2O, 0.8 g of K2HPO4, 1.0 g of NH4NO3, 0.2 g of MgSO4 · 7H2O, 10 mg of FeSO4 · 7H2O, 40 mg of MnCl2 · 4H2O, 0.1 g of ZnSO4 · 7H2O, and 0.5 g of yeast nitrogen base without amino acids (Difco) (pH 7.0). A soil sample was introduced into a 500-ml shaking flask containing the medium described above and incubated with shaking at 28°C for 7 days. Subsequently, 5 ml of the culture was transferred to another vessel containing fresh medium. After the enrichment culture was transferred five times, a pure culture was obtained from a single colony on an agar plate containing YT medium (10 g of Bacto Yeast Extract [Difco] per liter, 16 g of Bacto Tryptone [Difco]per liter, 5 g of NaCl per liter; pH 7.0).

Bacterial strains, culture conditions, and vectors. Strain P101, which was isolated from a soil sample as described above, was used in this work. This strain was most closely related to members of the genus Mycobacterium based on 16S RNA sequence analysis, which was conducted as described by Hiraishi et al. (14, 15). The results of morphological and physiological characterization were obtained from NCIMB Japan (Shimizu, Japan). Mycobacterium sp. strain P101 was grown at 28°C with shaking on NA medium to which a hydrocarbon (0.5%, vol/vol) was added as the carbon source.

Escherichia coli DH5{alpha} (TaKaRa, Kyoto, Japan), JM109, and Rosetta(DE3) (Novagen) were used for gene cloning and expression and were usually grown on YT medium or in Luria-Bertani (LB) broth, which contained 1% Bacto Tryptone, 0.5% Bacto Yeast Extract, and 0.5% NaCl (pH 7.0), in the presence of antibiotics when necessary. Plasmids and primers used in this work are listed in Table 1.


View this table:
[in this window]
[in a new window]
  		TABLE 1. Plasmids and primers used in this study

 
Analytical methods. Protein was measured with a Bio-Rad protein assay kit (Japan Bio-Rad Laboratories, Tokyo, Japan) with bovine serum albumin as the standard (6). Sodium dodecyl sulfate (SDS)-polyacrylamide gel electrophoresis (PAGE) was performed with a 12.5% polyacrylamide gel (19). Prestained protein markers (low range) for SDS-PAGE (Nacalai Tesque, Kyoto, Japan) were used as the molecular standards. The relative molecular masses of the native and SDS-denatured enzyme and the N-terminal amino acid sequence were determined as described previously (17). n-Alkanes and methyl-branched alkanes were determined by gas chromatography (GC7-A; Shimadzu Co. Ltd., Kyoto, Japan) under the following conditions: column, Ultra Alloy-1(HT) capillary column (Frontier Lab, Fukushima, Japan); column temperature gradient, 170 to 399°C; and temperature of injection port and flame ionization detector, 399°C. Gas chromatography-mass spectrometry (GC6890 and MS5973N; Agilent) was performed under the following conditions: gas chromatography with a TC-FFAP column (30 m by 0.25 mm; 0.5 µm; GLC Science, Tokyo, Japan) at 110 to 240°C for 20 min; and QUAD mass spectrometry at 80 eV, 230°C, and m/z 40 to 500.

Enzyme assays. The activity of {alpha}-methylacyl-CoA racemase (2-methylacyl-CoA epimerase; EC 5.1.99.4) was assayed by monitoring the conversion of (R)-2-methylpentadecanoyl-CoA to the (S) isomer (35) by gas chromatographic analysis of the fatty acid released by acidic hydrolysis of the CoA ester and condensed with (R)-1-phenylethylamine (10). The malate synthase (Mls; EC 4.1.3.2) activity was determined by a previously described method (25).

DNA sequencing. DNA sequencing was performed by the dideoxy chain termination method by using a Thermosequenase fluorescently labeled primer cycle sequencing kit with 7-deaza-dGTP (Amersham Bioscience K.K., Tokyo, Japan) and a DSQ-1000L DNA sequencer (Shimadzu Co. Ltd.).

Transposon mutagenesis. Preparation of cells for electroporation and transposon mutagenesis was carried out principally by using the methods described previously for strains belonging to the genus Rhodococcus (12). Electrocompetent cells (30 µl) of Mycobacterium sp. strain P101 were placed on ice in a 0.1-ml electrode gap Bio-Rad electroporation cuvette and mixed with 1.5 µg of the transposon Tn5-carrying plasmid pSUP10141 (30). After electroporation at 1.6 kV, 25 µF, and 300 {Omega}, the cells were resuspended in 1 ml of 2x YT medium and incubated overnight at 28°C. Aliquots of the culture were spread on LB medium plates containing neomycin at a concentration of 10 µg/ml and incubated at 28°C for 5 days. Colonies from the LB medium plates were patched onto NA agar plates, and growth was assayed with pristane or n-hexadecane vapor. The colonies on LB medium plates that could not grow on pristane or n-hexadecane on NA agar plates were rechecked for utilization of these carbon sources in liquid culture. Mutant strains P1 and H1, which were defective for growth on pristane and n-hexadecane, respectively, were selected for further characterization.

To confirm Tn5 insertion, chromosomal DNA was prepared from neomycin-resistant colonies and was digested to completion with EcoRI. Southern blot analysis was performed by using the neomycin resistance gene as a probe, and the probe was alkaline phosphatase labeled by using Alkphos direct labeling reagents (Amersham Bioscience K.K.). Hybridization was carried out at 55°C.

Cloning of the mutation in Mycobacterium sp. P101 and analysis of the surrounding DNA sequence. To determine the site of Tn5 insertion in mutant strains P1 and H1, total DNA from these strains was digested with ClaI. The ClaI DNA fragments were ligated into pBluescript II SK(+), and E. coli DH5{alpha} cells were transformed with the ligation mixture. The transformants were selected on LB agar plates containing ampicillin (50 µg/ml), 5-bromo-4-chloro-3-indolyl-ß-D-galactopyranoside (X-Gal) (20 µg/ml), and neomycin (50 µg/ml). DNA sequences of the insertions in the resulting plasmids, pTnP1 and pTnH1, derived from strains P1 and H1, respectively, were determined. Strain P1 was found to have a Tn5 insertion in a putative racemase gene (mcr) with 47% similarity to the gene encoding human {alpha}-methylacyl-CoA racemase (accession no. Q9UHK6). Strain H1 was shown to have a Tn5 insertion in a putative malate synthase gene (mls) with 83% similarity to the gene encoding malate synthase in M. tuberculosis (accession no. Q50596).

Cloning and nucleotide sequencing of mcr and mls genes. To obtain the complete mcr and mls genes from strain P101, colony hybridizations were performed. Hybridization probes for the mcr and mls genes were PCR amplified by using primers race-5 and race-3 and primers malate-5 and malate-3, respectively. Southern analysis of the genomic DNA from strain P101 showed that a 4.5-kb EcoRI-KpnI fragment hybridized to the probe for the mcr gene and a 3.8-kb BamHI-EcoRI fragment hybridized to the probe for the mls gene. Appropriate restriction enzyme-digested fragments from strain P101 were ligated into pBluescript II SK(+) and used to transform E. coli DH5{alpha}. Colony hybridizations were performed as described previously (32). Clones that showed strong signals were picked from the original plates, and the sequences of the corresponding plasmids, pYuR and pYuM, were determined.

Real-time quantitative reverse transcriptase PCR. Mycobacterium sp. strain P101 was cultured at 28°C on NA medium containing an appropriate carbon source to the early exponential phase and harvested. Total cellular RNA was extracted with an RNeasy mini kit (QIAGEN, Hilden, Germany) used according to the manufacturer's protocol. cDNA was synthesized in a 20-µl (final volume) mixture that included 5 µg of total RNA by using ReverTra Ace (Toyobo Co., Ltd., Osaka Japan) according to the manufacturer's instructions. Primer mcr-r (5 pmol) was used as the primer to amplify cDNA corresponding to the putative mcr gene. After reverse transcription for 50 min at 42°C, the sample was heated for 5 min at 99°C to terminate the reaction, and 0.5 µl of RNase H was added. Real-time quantitative PCR was performed in 20-µl (final volume) mixtures in glass capillary tubes in a LightCycler (Roche Diagnostic, Basel, Switzerland) (40). The PCR master mixture contained 3 mM MgCl2, 0.5 pmol of each primer, and 1x LightCycler-DNA Master SYBR Green I (Roche Diagnostics). Primers mcr-RTF and mcr-RTr were used to detect the mcr transcript. PCR amplification was performed as described previously (29). Amplicon specificity was verified by melting curve analyses conducted at 65 to 95°C (temperature transition, 0.1°C/s) with stepwise fluorescence acquisition and by ethidium bromide staining on 2% agarose gels. No fluorescence was detected by real-time quantitative PCR amplification without a template.

Purification of Mcr from E. coli Rosetta(DE3)(pET-R). To amplify the full-length open reading frame (ORF) fragment of the mcr gene, PCRs were performed by using pYuR as the template and primers mcr-oe-f and mcr-oe-r. The amplified fragments were digested with NdeI and HindIII and then ligated to pET-23a(+) (Novagen), yielding pET-R. E. coli Rosetta(DE3) was transformed with pET-R, and the resulting strain was grown in 2 liters of LB medium containing ampicillin (50 µg/ml) and chloramphenicol (34 µg/ml). When the culture reached an optical density at 610 nm of 0.6, isopropyl-ß-D-thiogalactopyranoside (IPTG) (4 mM) was added, and then the culture was incubated for an additional 6 h. The cells were harvested, washed with buffer A (50 mM potassium phosphate buffer containing 300 mM NaCl and 0.01% NaN3, pH 8.0), disrupted by sonication for 30 min (180 W; Insonator model 210 M; Kubota, Tokyo, Japan), and centrifuged at 5,600 x g for 15 min at 4°C and then at 40,000 x g for 1 h at 4°C. To the resultant clear supernatant, ammonium sulfate was added to a concentration of 1.2 M, and the sample was centrifuged. The resultant supernatant was applied to a Butyl-Toyopearl 650 M column (2.3 by 20 cm; Tosoh, Tokyo, Japan) that was preequilibrated with buffer A containing 1.2 M ammonium sulfate and then eluted with a linear gradient containing decreasing ammonium sulfate concentrations (1.2 to 0 M) in buffer A. The fractions containing the 39-kDa protein, as determined by SDS-PAGE, were collected, dialyzed against buffer B (10 mM potassium phosphate buffer containing 0.01% NaN3, pH 6.0), and then applied to a DEAE-Toyopearl 650 column (2.2 by 20 cm; Tosoh) preequilibrated with buffer B. Proteins were eluted with a linear gradient containing increasing concentrations of NaCl (0 to 0.5 M). The fractions exhibiting a single protein band at 39 kDa on an SDS-PAGE gel were collected and dialyzed against buffer B. The purified protein was used for the Mcr activity assay.

Expression of Mls protein in E. coli. To amplify the full-length ORF fragment of the mls gene, PCRs were performed by using pYuM as the template and primers mlsoe-f and mlsoe-r. The amplified fragments were digested with NdeI and EcoRI and then ligated to pET-23a(+), yielding pET-M. E. coli Rosetta(DE3) was transformed with pET-M, and the resulting strain was grown in 50 ml of LB medium containing ampicillin (50 µg/ml) and chloramphenicol (34 µg/ml).

Whole-cell reactions. Cells were grown in NA medium containing acetic acid (1 g/liter) as the carbon source for 3 days, harvested, and washed with cold water. The washed cells (12 mg [dry weight]) were inoculated into 1.0 ml of NA medium with a carbon source (0.5%, vol/vol) in the absence of NH4NO3 as the nitrogen source. The whole-cell reactions were conducted in 50-ml anaerobic culture tubes (Bellco Glass Inc.) with butyl gum stoppers with shaking at 28°C. The volume of air in each tube was sufficient for oxidation of the amount of substrate added. A portion of each reaction mixture was removed, and the whole samples containing the cells were extracted with ethyl acetate under acidic conditions (pH less than 2.0). The extracts were subjected to gas chromatography-mass spectrometry as described above.

Nucleotide sequence accession numbers. The nucleotide sequences have been deposited in the GenBank database under the following accession numbers: 16S ribosomal DNA sequence of strain P101, AB182286; 4.7-kb EcoRI-KpnI fragment, AB182284; and EcoRI-BamHI fragment, AB182285.


   RESULTS
Top
 Abstract
 Introduction
 Materials and Methods
 Results
Discussion
 References
 
Properties of newly isolated strain P101. The new isolate, strain P101, was able to grow on methyl-branched alkanes (pristane, phytane, and squalane) and n-alkanes (C5, C6, and C11 to C18) as sole sources of carbon but could not grow on iso-octane, 2,2,4,4,6,8,8-heptamethylnonane, and aromatic hydrocarbons, such as benzene, toluene, p-xylene, naphthalene, and phenanthrene. Strain P101 was a high-G+C-content mycolic-acid containing gram-positive bacterium and was most closely related to members of the genus Mycobacterium on the basis of 16S ribosomal DNA sequencing. The highest level of similarity (99.5% identity) was found with the sequence of Mycobacterium fluoranthenicum.

Figure 1 shows growth of strain P101 on NA medium containing pristane and n-hexadecane as the carbon sources. The organism completely degraded 0.5% (vol/vol) n-hexadecane within 36 h, and it took longer (60 h) to consume 0.5% (vol/vol) pristane. In the presence of both substrates, degradation of pristane followed degradation of n-hexadecane, but the degradation rates for each substrate were almost the same as those when each substrate was used as the sole carbon source. Pristane utilization occurred before n-hexadecane was completely consumed, meaning that degradation of the two substrates occurred simultaneously, and neither substrate inhibited growth on the other substrate.



View larger version (21K):
[in this window]
[in a new window]
  		FIG. 1. Growth of Mycobacterium sp. strain P101 on pristane (A), n-hexadecane (B), and pristane and n-hexadecane (C). Pristane ({blacksquare}) and n-hexadecane ({square}) were added at a concentration of 0.5% (vol/vol) to NA medium. {circ}, growth.

 
Isolation of mutants deficient in the ability to grow on pristane or n-hexadecane. About 10,000 neomycin-resistant mutants were obtained by Tn5 mutagenesis by using pSUP10141. To confirm insertion of the transposon, chromosomal DNA was prepared from 83 selected transposon-containing colonies. The EcoRI-digested genomic DNA isolated from the mutants were subjected to Southern blot analyses by using a 1-kb DNA fragment amplified from the Tn5 Nmr gene sequence as the probe. These Southern blot analyses revealed that random insertion of Tn5 occurred in strain P101. Eighty of the mutants were unable to grow on both pristane and n-hexadecane but grew on NA medium containing succinate as a carbon source, implying that some common gene products participate in pathways for both the methyl-branched alkanes and n-alkanes. Two mutants (P1 and P2) were not capable of growth on methyl-branched alkanes (pristane, phytane, and squalane), but they grew on n-hexadecane at the same rate as the parent strain. The restriction profiles and recovered sequences around the inserted Tn5 were identical for mutants P1 and P2, indicating that they were siblings (data not shown). Another mutant strain, H1, was not capable of growth on n-hexadecane and partially retained the ability to grow on pristane. Southern analyses of the mutants indicated that each mutant contained a single Tn5 insertion in the chromosome.

Determination of Tn5 insertion loci. The 6.5-kb ClaI fragment from the chromosomal DNA of mutant P1 and the 6.6-kb ClaI fragment from mutant H1 were subcloned into pBluescriptII SK(+) to obtain plasmids pTnP1 and pTnH1, respectively. DNA sequence analyses of these plasmids revealed that the Tn5 insertion disrupted a gene with high sequence similarity to the {alpha}-methylacyl-CoA racemase gene (mcr) in mutant P1 and the malate synthase gene (mls) in mutant H1.

Cloning and sequencing of native genomic fragments. A 4.7-kb EcoRI-KpnI fragment of plasmid pYuR, which was obtained through colony hybridization selection by using an mcr DNA fragment as the probe, contained three complete ORFs and one partial ORF (Fig. 2). The sequence of orf2 matched the sequence of the mcr gene of mutant P1, into which Tn5 was inserted. The native mcr gene was composed of 1,083 bp, corresponding to 361 amino acid residues with a predicted molecular mass of 38,867 Da. Mcr showed considerable similarity to {alpha}-methylacyl-CoA racemases from different sources. From the results of BLAST searches, the products of orf1 and orf3 were aligned with 2-enoyl-CoA hydratase and 3-hydroxyacyl-CoA dehydrogenase, respectively (Fig. 2). These enzymes participate in bacterial ß-oxidation (24).



View larger version (34K):
[in this window]
[in a new window]
  		FIG. 2. Gene organization and restriction maps of the fragments carrying mcr and mls. (A) 6.3-kb gene region of Mycobacterium sp. strain P101. (B) 3.8-kb gene region of Mycobacterium sp. strain P101. (C) Southern analysis of ClaI-digested total DNA from the wild-type strain and mutant strain P1, with the alkaline phosphatase-labeled mcr fragment as a probe. (D) Southern analysis of ClaI-digested total DNA from the wild-type strain and mutant strain H1, with the alkaline phosphatase-labeled mls fragment as a probe. Based on the results of BLAST searches, the ORFs showed amino acid sequence similarity to the following known proteins: for orf1 (829 bp), 2-enoyl-CoA hydratase from Azoarcus evansii (accession no. AJ278756; 28% identity and 44% similarity); for orf2 (1,083 bp), {alpha}-methylacyl-CoA racemase; for orf3 (729 bp), 3-hydroxyacyl-CoA dehydrogenase from Pseudomonas putida (accession no. Q9AHY1; 52% identity and 67% similarity); and for orf4 (partial), 2-nitropropane dioxygenase from Streptomyces ansochromogenes (accession no. AF284037; 22% identity and 34% similarity). The product of a partial orf6 was similar to a putative protein found in M. tuberculosis (accession no.Q50597).

 
A 3.8-kb BamHI-EcoRI fragment of plasmid pYuM, which was obtained by using mls DNA as the hybridization probe, contained a partial ORF (orf6) and a complete ORF (orf5) (Fig. 2). orf5 was composed of 2,211 bp, corresponding to 737 amino acid residues with a predicted molecular mass of 79,587 Da. orf5 was identical to the mls gene from mutant H1, into which Tn5 was inserted. Mls showed considerable similarity to malate synthases from different sources.

Enzymatic activities of Mcr and Mls. Mcr protein (1.2 mg) was purified from the cell extract of E. coli Rosetta(DE3)(pET-R) (330 mg of protein). The N-terminal amino acid sequence was MTGPLHG, which was identical to the deduced amino acid sequence of ORF2. The relative molecular mass of the purified Mcr was estimated to be 39 kDa by SDS-PAGE, which was in good agreement with the theoretical molecular mass, as described above. The purified enzyme was confirmed to catalyze partial conversion of (R)-2-methylpentadecanoyl-CoA to the corresponding (S) isomer. The specific activity of the purified enzyme was 0.21 µmol · min–1 · mg of protein–1.

SDS-PAGE of the cell extract of E. coli Rosetta(DE3) (pET-M) revealed a major protein band, whose molecular mass (80 kDa) was in close agreement with the theoretical mass of the deduced amino acid sequence of the mls gene product. The N-terminal amino acid sequence of the protein was MTERVTV, which was identical to the deduced amino acid sequence. The cell extract exhibited a malate synthase activity of 6.49 µmol · min–1 · mg of protein–1. The malate synthase activity of the control strain harboring pET-23a(+) was less than 1% of that of E. coli Rosetta(DE3)(pET-M).

Transcription analysis. To characterize the transcriptional regulation of the mcr gene, real-time quantitative reverse transcriptase PCR was conducted with total RNA from strain P101 cells, which were grown on NA medium containing pristane, phytane, squalane, n-hexadecane, or succinate. The results suggested that the mcr expression in the presence of pristane and squalane was induced 9.1- and 3.4-fold relative to that in the presence of succinate, respectively. Since the control reverse transcription experiment did not produce fluorescence within a reasonable number of cycles (data not shown), mcr was suggested to be transcribed constitutively.

Growth characteristics of mutant strains P1 and H1. In order to determine the physiological role of Mcr in the utilization of methyl-branched alkanes, growth of wild-type strain P101 and growth of the mcr-deficient mutant strain P1 on several carbon sources were compared. Although strain P1 could not grow on pristane as a sole source of carbon, it grew on NA medium containing both pristane (0 to 0.3%, wt/vol) and n-hexadecane (0.5%) (Fig. 3). There was no significant change in the extent of growth of strain P1, even when the concentration of pristane was increased. This extent of growth was almost the same as that observed in the absence of pristane. These results indicated that the growth of strain P1 was sustained by n-hexadecane and also suggested that pristane or its metabolic intermediates were not toxic for growth of the mutant strain on n-hexadecane. In order to determine the stereospecificity of the enzyme for 2-methyl-branched fatty acids, 2-methylbutyric acid (1.0%, wt/vol) was used as the growth substrate. Among the methyl-branched fatty acids, only the (S)-2-methylbutyric acid stereoisomer was commercially available. The wild-type strain was able to grow on the racemic compound, as well as the (S) isomer. Mutant P1 consumed the (S) isomer within 5 days, and the growth yield was 2.2 g (dry weight)/liter; however, mutant P1 did not grow on the racemic compound, (R,S)-2-methylbutyric acid. These results imply that the mcr-deficient mutant is able to use only the (S) isomer of the 2-methyl-branched fatty acid and that the (R) isomer, or a derivative of it, inhibits utilization of the (S) isomer.



View larger version (24K):
[in this window]
[in a new window]
  		FIG. 3. Growth of wild-type strain P101 and mcr-deficient mutant strain P1 on NA media containing pristane and n-hexadecane. (A) Growth on pristane as the carbon source at the concentrations indicated. (B) Growth on 0.5% n-hexadecane and pristane at the concentrations indicated. The open and solid bars show the growth of strains P101 and P1, respectively, after 3 days of cultivation. Experiments were done in triplicate, and the error bars indicate the observed standard deviations. dcw, dry weight of cells.

 
The mls mutant strain H1 had consumed about 70% of the added pristane (1.5 g/liter) after 3 days of cultivation, and the cell yield based on the amount of pristane consumed was 27%, which corresponded to 58% of the cell yield of the wild-type strain.

Pristanic acid accumulation from pristane by mutant strain P1. The consumption of pristane and n-hexadecane in whole-cell reactions with the mutant and wild-type strains was investigated. The wild-type strain completely consumed both n-hexadecane and pristane (1 g/liter each) during a 24-h incubation at 28°C. Mutant strain P1 consumed n-hexadecane at the same rate as the wild-type strain. On the other hand, about 5% of the added pristane was consumed in the reaction with the mutant strain. Only one significant peak corresponding to pristanic acid was detected on the gas chromatograph of the ethyl acetate extract, and the amount accumulated reached a maximum (0.08 mM in the reaction mixture) after 72 h of incubation (data not shown). This peak was not detected with the reaction mixture containing the wild-type strain. The mass spectrographic data for this peak matched the data for authentic pristanoic acid (m/z 43, 57, 74, 87, 99, 115, 127, and 298 [molecular ion]). Since the reaction mixture was treated under acidic conditions, pristanic acid may have been derived from pristanoyl-CoA (a possible intermediate in pristane oxidation) by acid hydrolysis.


   DISCUSSION
Top
 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
References
 
A pathway for oxidation of pristane in some gram-positive bacteria has been proposed based on an analysis of key intermediates. However, the relevant enzymes have not been characterized yet. In this work, we found that {alpha}-methylacyl-CoA racemase plays a critical role in the complete oxidation of pristane in Mycobacterium sp. strain P101. Bacterial ß-oxidation of branched fatty acids has been proposed to proceed through an analogous route in mammalian cells. Our findings provide corroborating evidence for the proposed pathway for pristane oxidation and call attention to the stereospecific aspects of the ß-oxidation pathway.

In mammalian cells, stereospecific enzymatic recognition occurs in the steps for desaturation of the acyl-CoA through ß-oxidation, which are catalyzed by acyl-CoA oxidase in the peroxisome (35) and acyl-CoA dehydrogenase in the mitochondrion (24). Since these enzymes are specific for (S)-2-methylacyl-CoA, {alpha}-methylacyl-CoA racemase is indispensable for completion of ß-oxidation. In bacteria, desaturation of acyl-CoAs is catalyzed by acyl-CoA dehydrogenase (24). We suggest that this desaturation step is stereospecific for the (S) configuration and that the (R) isomer inhibits the desaturation step based on the following results: (i) the mcr-deficient mutant of strain P101 used (S)-2-methylbutyric acid but not the racemic compound, and (ii) pristanic acid, which may be derived from pristanoyl-CoA, was detected as a dead-end product of pristane oxidation by the mutant. Judging from the evidence that n-hexadecane utilization by the mutant is not inhibited by pristane, the unmetabolized isomer, (R)-2-methylacyl-CoA, is not toxic for ß-oxidation of unbranched fatty acids. This may imply that different desaturation enzymes function with 2-methylated acyl-CoAs and unmethylated acyl-CoAs.

Based on previous reports for M. fortuitum (9) and N. globerula 432 (1), Mycobacterium sp. strain P101 was assumed to oxidize pristane through monoterminal oxidation; i.e., pristanic acid is thioesterified with CoA to form pristanoyl-CoA and then degraded by ß-oxidation. The pristane used in this work was derived from shark liver oil, which is composed of only the (6R,10S)-meso isomer (8). Oxidation of the isomers of pristane (compound I) is expected to produce the following four isomers of pristanic acid: (2R,6R,10R), (2S,6R,10R), (2R,6S,10S), and (2S,6S,10S) (Fig. 4). Assuming that the configurations of the CoA thioesters are the same as those of the corresponding acids, compounds III, V, VII, and IX should be substrates for Mcr. Three mcr homologues are present in the M. tuberculosis genome (5), although the physiological role of each gene product has not been elucidated. In Mycobacterium sp. strain P101, Southern blot analysis identified only one gene for the enzyme (mcr) in the entire genome (data not shown), indicating that Mcr is responsible for racemization of compounds III, V, VII, and IX. Also, the gene arrangement in the vicinity of the mcr gene was completely different in strain P101 and M. tuberculosis.



View larger version (22K):
[in this window]
[in a new window]
  		FIG. 4. Proposed ß-oxidation pathway for pristane in Mycobacterium sp. strain P101. Three moles of propionyl-CoA, 3 mol of acetyl-CoA, and 1 mol of isobutyryl-CoA are produced from 1 mol of pristane. R and S indicate the possible configuration of each asymmetric carbon. For example, compound II consists of four stereoisomers, (2R,6R,10R), (2S,6R,10R), (2R,6S,10S), and (2S,6S,10S).

 
As shown in Fig. 4, three equivalents of propionyl-CoA, three equivalents of acetyl-CoA, and one equivalent of isobutyryl-CoA can be produced from 1 mol of pristane. Propionyl-CoA is thought to be incorporated into cell constituents through the 2-methylcitric acid cycle that occurs in a variety of bacteria (7, 16, 20, 33). Thus, the mls-deficient mutant should obtain cell carbon through propionyl-CoA and isobutyryl-CoA in an amount corresponding to 12/19 of that of the wild-type strain, which can utilize all acyl-CoAs, if the cell yield is estimated on the basis of available carbon number. When the cell yields based on pristane consumption were compared, the yield for the mutant was 58% of the yield obtained with the wild type, implying that pathways for pristane and n-alkane degradation function independently in the bacterium.

Bacterial metabolism of branched-chain fatty acids has received little attention compared with mammalian metabolism. Further work is needed to clarify whether enzymatic discrimination between branched-chain acyl-CoAs and straight-chain acyl-CoAs occurs in the ß-oxidation pathway. Some members of the order Actinomycetales, such as Rhodococcus, Nocardia, Mycobacterium, etc., are known to use a variety of hydrocarbons, including methyl-branched alkanes, and have different gene clusters for oxidation of alkanes with different chain lengths (13, 17, 31, 39). Attention should also be focused on the enzymatic discrimination between iso-alkanes and n-alkanes in their oxidation to the corresponding fatty acids.


   ACKNOWLEDGMENTS
 
This research was supported in part by grant-in-aid for scientific research (S) 13854008 to Y.S. This work was also supported in part by COE for Microbial-Process Development Pioneering Future Production Systems (COE program of the Ministry of Education, Culture, Sports, Science and Technology, Japan). The work in Leuven was supported by grant GOA 2004/08 from the Flemish government.


   FOOTNOTES
 
* Corresponding author. Mailing address: Division of Applied Life Sciences, Graduate School of Agriculture, Kyoto University, Kitashirakawa, Sakyo-ku, Kyoto 606-8502, Japan. Phone: 81 75 753 6385. Fax: 81 75 753 6385. E-mail: nkato{at}kais.kyoto-u.ac.jp. Back


   REFERENCES
Top
 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
 References
 

  1. Alvarez, H. M., M. F. Souto, A. Viale, and O. H. Pucci. 2001. Biosynthesis of fatty acids and triacylglycerols by 2,6,10,14-tetramethyl pentadecane-grown cells of Nocardica globerula 432. FEMS Microbiol. Lett. 200:195-200.[CrossRef][Medline]
  2. Amery, L., M. Fransen, K. de Nys, G. P. Mannaerts, and P. P. Van Veldhoven. 2000. Mitochondrial and peroxisomal targeting of 2-methylacyl-CoA racemase in humans. J. Lipid Res. 41:1752-1759.[Abstract/Free Full Text]
  3. Atlas, R. M. 1981. Microbial degradation of petroleum hydrocarbons: an environmental perspective. Microbiol. Rev. 45:180-209.[Free Full Text]
  4. Berthou, F., and M. P. Friocourt. 1981. Gas chromatographic separation of diastereomeric isoprenoids as molecular markers of oil pollution. J. Chromatogr. 219:393-402.[Medline]
  5. Bhaumik, P., P. Kursula, V. Ratas, E. Conzelmann, J. K. Hiltunen, W. Schmitz, and R. K. Wierenga. 2003. Crystallization and preliminary X-ray diffraction studies of an {alpha}-methylacyl-CoA racemase from Mycobacterium tuberculosis. Acta Crystallogr. Sect. D Biol. Crystallogr. 59:353-355.[CrossRef][Medline]
  6. Bradford, M. M. 1976. A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal. Biochem. 72:248-254.[CrossRef][Medline]
  7. Clases, W. A., A. Puhler, and J. Kalinowski. 2002. Identification of two prpDBC gene clusters in Corynebacterium glutamicum and their involvement in propionate degradation via the 2-methylcitrate cycle. J. Bacteriol. 184:2728-2739.[Abstract/Free Full Text]
  8. Cox, R. E., J. R. Maxwell, R. G. Ackman, and S. N. Hooper. 1972. Stereochemical studies of acyclic isoprenoid compounds. III. The stereochemistry of naturally occurring (marine) 2,6,10,14-tetramethylpentadecane. Can. J. Biochem. 50:1238-1241.[Medline]
  9. Cox, R. E., J. R. Maxwell, R. G. Ackman, and S. N. Hooper. 1974. Stereochemical studies of acyclic isoprenoid compounds. IV. Microbial oxidation of 2,6,10,14-tetramethylpentadecane (pristane). Biochim. Biophys. Acta 360:166-173.[Medline]
  10. Croes, K., M. Casteels, M. Dieuaide-Noubhani, G. P. Mannaerts, and P. P. Van Veldhoven. 1999. Stereochemistry of the alpha-oxidation of 3-methyl-branched fatty acid in rat liver. J. Lipid Res. 40:601-609.[Abstract/Free Full Text]
  11. Ferdinandusse, S., S. Denis, L. Ijlst, G. Dacremont, H. R. Waterham, and R. J. A. Wanders. 2000. Subcellular localization and physiological role of {alpha}-methylacyl-CoA racemase. J. Lipid Res. 41:1890-1896.[Abstract/Free Full Text]
  12. Fernandes, P. J., J. A. C. Powell, and J. A. C. Archer. 2001. Construction of Rhodococcus random mutagenesis libraries using Tn5 transposition complexes. Microbiology 147:2529-2536.[Abstract/Free Full Text]
  13. Hamamura, N., C. M. Yeager, and D. J. Arp. 2001. Two distinct monooxygenases for alkane oxidation in Nocardioides sp. strain CF8. Appl. Environ. Microbiol. 67:4992-4998.[Abstract/Free Full Text]
  14. Hiraishi, A. 1992. Direct automated sequencing of 16S rDNA amplified by polymerase chain reaction from bacterial cultures without DNA purification. Lett. Appl. Microbiol. 15:210-213.[Medline]
  15. Hiraishi, A., Y. K. Shin, Y. Ueda, and J. Sugiyama. 1994. Automated sequencing of PCR-amplified 16S rDNA on 'Hydrolink' gels. J. Microbiol. Methods 19:145-154.
  16. Horswill, A. R., and J. C. Escalante-Semerena. 1999. Salmonella typhimurium LT2 catabolizes propionate via the 2-methylcitric acid cycle. J. Bacteriol. 181:5615-5623.[Abstract/Free Full Text]
  17. Kotani, T., T. Yamamoto, H. Yurimoto, Y. Sakai, and N. Kato. 2003. Propane monooxygenase and NAD+-dependent secondary alcohol dehydrogenase in propane metabolism by Gordonia sp. strain TY-5. J. Bacteriol. 185:7120-7128.[Abstract/Free Full Text]
  18. Kotti, T. J., K. Savolaninen, H. M. Helander, A. Yagi, D. K. Novikov, N. Kakllinen, E. Conzelmann, J. K. Hiltunen, and W. Schmitz. 2000. In mouse {alpha}-methylacyl-CoA racemase, the same gene product is simultaneously located in mitochondria and peroxisomes. J. Biol. Chem. 275:20887-20895.[Abstract/Free Full Text]
  19. Laemmli, U. K. 1970. Cleavage of structural proteins during the assembly of the head of bacteriophage T4. Nature 227:680-685.[CrossRef][Medline]
  20. London, R. E., D. L. Allen, S. A. Gabel, and E. F. DeRose. 1999. Carbon-13 nuclear magnetic resonance study of metabolism of propionate by Escherichia coli. J. Bacteriol. 181:3562-3570.[Abstract/Free Full Text]
  21. Lough, A. K. 1967. The occurrence of diastereoiomers of phytanic acid and pristanic acid and their determination by gas-liquid chromatography. Lipids 2:357-362.[Medline]
  22. McKenna, E. J., and R. E. Kallio. 1971. Microbial metabolism of the isoprenoid alkane pristane. Proc. Natl. Acad. Sci. USA 68:1552-1554.[Abstract/Free Full Text]
  23. Nakajima, K., and A. Sato. 1983. Microbial metabolism of the isoprenoid alkane pristane. Nippon Nogeikagaku Kaishi 57:299-305.
  24. Nunn, W. D. 1986. A molecular view of fatty acid catabolism in Escherichia coli. Microbiol. Rev. 50:179-192.[Free Full Text]
  25. Ornston, L. N., and M. K. Ornston. 1969. Regulation of glyoxylate metabolism in Escherichia coli K-12. J. Bacteriol. 98:1098-1108.[Abstract/Free Full Text]
  26. Pirnik, M. P., R. M. Atlas, and R. Bartha. 1974. Hydrocarbon metabolism by Brevibacterium erythrogenes: normal and branched alkanes. J. Bacteriol. 119:868-878.[Abstract/Free Full Text]
  27. Schmitz, W., C. Albers, R. Fingerhut, and E. Conzelmann. 1995. Purification and characterization of an {alpha}-methyl-CoA racemase from human liver. Eur. J. Biochem. 231:815-822.[Medline]
  28. Schmitz, W., R. Fingerhut, and E. Conzelmann. 1994. Purification and properties of an {alpha}-methylacyl-CoA racemase from rat liver. Eur. J. Biochem. 222:313-323.[Medline]
  29. Shinoda, Y., Y. Sakai, H. Uenishi, Y. Uchihashi, A. Hiraishi, H. Yukawa, H. Yurimoto, and N. Kato. 2004. Aerobic and anaerobic toluene degradation by a newly isolated denitrifying bacterium, Thauera sp. strain DNT-1. Appl. Environ. Microbiol. 70:1385-1392.[Abstract/Free Full Text]
  30. Simon, R., U. Priefer, and A. Puehler. 1983. A broad host range mobilization system for in vivo genetic engineering: transposon mutagenesis in gram negative bacteria. Bio/Technology 1:784-791.[CrossRef]
  31. Smits, T. H., S. B. Balada, B. Witholt, and J. B. van Beilen. 2002. Functional analysis of alkane hydroxylases from gram-positive bacteria. J. Bacteriol. 184:1733-1742.[Abstract/Free Full Text]
  32. Tani, A., T. Ishige, Y. Sakai, and N. Kato. 2001. Gene structures and regulation of the alkane hydroxylase complex in Acinetobacter sp. strain M-1. J. Bacteriol. 183:1819-1823.[Abstract/Free Full Text]
  33. Textor, S., V. F. Wendish, A. A. De Graaf, U. Muller, M. I. Linder, D. Linder, and W. Buckel. 1997. Propionate oxidation in Escherichia coli: evidence for operation of a methylcitrate cycle in bacteria. Arch. Microbiol. 168:428-436.[CrossRef][Medline]
  34. van Hylckama Vlieg, J. E. T., H. Leemhuis, J. H. Lutje Spelberg, and D. B. Janssen. 2000. Characterization of the gene cluster involved in isoprene metabolism in Rhodococcus sp. strain AD45. J. Bacteriol. 182:1956-1963.[Abstract/Free Full Text]
  35. Van Veldhoven, P. P., K. Croes, S. Asselberghs, P. Herdewijn, and G. P. Mannaerts. 1996. Peroxisomal ß-oxidation of 2-methyl-branched acyl-CoA esters: stereospecific recognition of the 2S-methyl compounds by trihydroxycoprostanoyl-CoA oxidase and pristanoyl-CoA oxidase. FEBS Lett. 388:80-84.[CrossRef][Medline]
  36. Van Veldhoven, P. P., K. Croes, M. Casteels, and G. P. Mannaerts. 1997. 2-Methylacyl racemase: a coupled assay based on the use of pristanoyl-CoA/peroxidase and reinvestigation of its subcellular distribution in rat and human liver. Biochim. Biophys. Acta 1347:62-68.[Medline]
  37. Van Veldhoven, P. P., E. Meyni, R. H. Squires, M. Fransen, B. Fournier, V. Brys, M. J. Bennett, and G. P. Mannaerts. 2001. Fibroblast studies documenting a case of peroxisomal 2-methylacyl-CoA racemase deficiency: possible link between racemase deficiency and malabsorption and vitamin K deficiency. Eur. J. Clin. Investig. 31:714-722.[CrossRef][Medline]
  38. Verhoeven, N. M., and C. Jakobs. 2001. Human metabolism of phytanic acid and pristanic acid. Prog. Lipid Res. 40:453-466.[CrossRef][Medline]
  39. Whyte, L. G., T. H. Smits, D. Labbe, B. Witholt, C. W. Greer, and J. B. van Beilen. 2002. Gene cloning and characterization of multiple alkane hydroxylase systems in Rhodococcus strains Q15 and NRRLB-16531. Appl. Environ. Microbiol. 68:5933-5942.[Abstract/Free Full Text]
  40. Wittwer, C. T., K. M. Ririe, R. V. Andrew, D. A. David, R. A. Gundry, and U. J. Balis. 1997. The LightCycler: a micovolume multisample fluorimeter with rapid temperature control. BioTechniques 22:176-181.[Medline]

Journal of Bacteriology, November 2004, p. 7214-7220, Vol. 186, No. 21
0021-9193/04/$08.00+0     DOI: 10.1128/JB.186.21.7214-7220.2004
Copyright © 2004, American Society for Microbiology. All Rights Reserved.



This article has been cited by other articles:


This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Services
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrow Copyright Information
Right arrow Books from ASM Press
Right arrow MicrobeWorld
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Sakai, Y.
Right arrow Articles by Kato, N.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Sakai, Y.
Right arrow Articles by Kato, N.

Home Help [Feedback] [For Subscribers] [Archive] [Search] [Contents]
Appl. Environ. Microbiol. Infect. Immun. Eukaryot. Cell
Mol. Cell. Biol. J. Virol. Microbiol. Mol. Biol. Rev.
ALL ASM JOURNALS