| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
1 Institut für Molekulare Mikrobiologie und Biotechnologie, Westfälische Wilhelms-Universität Münster, Corrensstraße 3, 48149 Münster, Germany
2 Laboratory of Microbiology, Department of Biochemistry, Physiology and Microbiology, University of Ghent, K. L. Ledeganckstraat 35, 9000 Ghent, Belgium
Correspondence
Alexander Steinbüchel
steinbu{at}uni-muenster.de
 |
ABSTRACT |
|---|
 TOP ABSTRACT MAIN TEXTREFERENCES |
|---|
The GenBank/EMBL/DDBJ accession number for the 16S rRNA gene sequence of strain DPN7T is AY880023.
A phase-contrast micrograph of cells of strain DPN7T is available as supplementary material in IJSEM Online.
Present addresss: Massachusetts Institute of Technology, Department of Chemical Engineering, 77 Massachusetts Avenue 56-422, Cambridge, MA 02139, USA. 
|
MAIN TEXT |
|---|
|
TOPABSTRACTMAIN TEXTREFERENCES |
|---|
). The first example of this novel type of biopolymer was found to be synthesized by Ralstonia eutropha, a Gram-negative soil bacterium, which naturally accumulates polyhydroxyalkanoates at levels up to more than 90 % of cell dry matter (Pedrós-Alio et al., 1985). R. eutropha can produce various polythioester copolymers under specific cultivation conditions in the presence of 3-mercaptopropionic acid, 3-mercaptovaleric acid, 3,3'-thiodipropionic acid or 3,3'-dithiodipropionic acid (DTDP) by employing its polyhydroxyalkanoate synthase (Lütke-Eversloh et al., 2001a, b; Lütke-Eversloh & Steinbüchel, 2003). Polythioester homopolymers were synthesized from 3-mercaptopropionic acid, 3-mercaptobutyric acid or 3-mercaptovaleric acid by a recombinant strain of Escherichia coli expressing a non-natural pathway (Lütke-Eversloh et al., 2002).
R. eutropha and E. coli are unable to utilize these sulfur-containing substrates as sole carbon sources for growth. In addition, polythioesters currently cannot be synthesized de novo from simple carbon sources and sulphate: their biosynthesis depends on the use of the organic sulfur compounds mentioned above. Little is known (or published) about the catabolic pathways of organic sulfur compounds; exceptions are the catabolism of cysteine and methionine as well that as of dimethylsulfoxide, dimethylsulfoniopropionate and dimethylsulfide as intermediates of the sulfur cycle (Kertesz, 2000; Kiene et al., 2000; Lomans et al., 2002; Yoch, 2002) and the biodesulfurization of benzothiophenes (McFarland, 1999) and of the fluorinated organic sulfur compound bis-(3-pentafluorophenylpropyl)-sulfide (Van Hamme et al., 2004).
To investigate the unknown catabolism of DTDP (Fig. 1), which is one of the precursor substrates currently used for the production of 3-mercaptopropionic acid-containing polythioesters (Lütke-Eversloh & Steinbüchel, 2003), bacterial strains capable of utilizing this organic sulfur compound as a carbon source for growth are desirable for the understanding, and potential application, of DTDP-converting enzymes. In this study, we describe the taxonomic and biochemical characterization of a newly isolated bacterium, strain DPN7T, which is able to grow with DTDP as the sole carbon source.
|
) supplemented with 0.5 % (w/v) DTDP as the sole carbon source with approximately 2 g compost. The culture was incubated at 30 °C for approximately 1 week. Afterwards, serial dilutions of the enrichment culture were spread onto MSM agar plates containing 0.5 % (w/v) DTDP and then incubated for 7 days at 30 °C. Cells from large colonies were repeatedly transferred to identical agar plates until an axenic culture was obtained. Storage was accomplished in screw-capped vials at –70 °C in 20 % (v/v) glycerol and as lyophilizates.
Colonies of strain DPN7T were circular, white to lime-yellowish in colour and were more flat than convex. Older colonies on MSM-DTDP agar developed a more yellowish colour. On complex medium, colonies of DPN7T grew in 1–2 days and appeared more white than yellow in colour. The cells were cultivated at 30 °C in liquid MSM containing 0.5 % (w/v) DTDP and samples were withdrawn from different growth stages of the culture. Cells of DPN7T were Gram-negative, coccoid rods approximately 1.5–2 µm in length and 1.5 µm in width and often occurred in pairs, as revealed under a Zeiss light microscope (see Supplementary Fig. S1 available in IJSEM Online). Cell motility was observed: after flagella staining performed according to Blenden & Goldberg (1964), one or two flagella could be detected.
Gram-staining performed according to Gerhardt et al. (1994) gave a negative reaction. Strain DPN7T was oxidase-positive, as revealed by using Bactident oxidase test strips (Merck), and was catalase-positive, as revealed by adding 3 % (v/v) H2O2 to freshly grown colonies. API 20NE (bioMérieux) was used to determine the assimilation of some carbon sources and the presence of important enzymes. The utilization of different carbon sources and the growth at different temperatures were investigated in liquid MSM and on MSM agar plates containing 0.2 % (w/v) of the respective carbon source (Table 1), unless indicated otherwise. Besides having the physiological characteristics shown in Table 1, both strains were positive for utilization of D-glucose, sodium gluconate, acetic acid, propionic acid, butyric acid and succinic acid by conventional cultivation and according to the API 20NE system both strains were positive for utilization of L-arabinose, adipic acid, citric acid and malic acid and negative for D-mannose, D-mannitol, D-maltose, N-acetylglucosamine, capric acid and phenylacetic acid. Additional biochemical characteristics (shown in Table 1) according to the API 20NE system were as follows: both strains were positive for urease activity and negative with regard to the fermentative degradation of glucose, indole production and activity of arginine dihydrolase, 
-glucosidase, protease and -galactosidase. This strain had no specific requirement for vitamins and also showed no enhanced growth in the presence of vitamin solution (Mohn, 1995) in defined medium. Growth was typically observed after 2–4 days on MSM agar plates containing 0.5 % (w/v) DTDP when incubated at 20–37 °C. In liquid MSM containing 0.2–0.5 % (w/v) DTDP as the sole carbon source, strain DPN7T exhibited a characteristic lag phase of approximately 48 h. After that period of time, the exponential phase followed, with a reproducible duration of more than 50 h. To the best of our knowledge, this is the first bacterial isolate found to utilize DTDP as the sole carbon and energy source for growth. Whereas good growth occurred with DTDP, no growth was observed with the C4 analogue 4,4'-dithiodibutyric acid or with 3,3'-thiodipropionic acid. The putative cleavage product of DTDP, 3-mercaptopropionic acid, could be utilized only at concentrations of less than 0.2 %, because of its toxicity (Table 1).
|
; Timm et al., 1990). The cells were capable of synthesizing poly(3-hydroxybutyrate) as a storage compound when they were cultivated in MSM containing gluconate as the sole carbon source. When DTDP or 3-mercaptopropionic acid was provided as an additional carbon source, the cells accumulated a copolymer (up to 20 mol%), consisting of 3-hydroxybutyrate and 3-mercaptopropionic acid.
Antibiotic-susceptibility testing on nutrient broth agar (Sambrook et al., 1989) containing different concentrations of antibiotics showed good growth of strain DPN7T on plates containing 5 µg chloramphenicol ml–1 and poor growth with 50 µg chloramphenicol ml–1, but no growth with 500 µg chloramphenicol ml–1. Growth also occurred in the presence of 50 µg thiostrepton ml–1. The strain showed no growth on plates containing 5 µg kanamycin ml–1, 5 µg gentamicin ml–1, 6.25 µg tetracycline ml–1 or 50 µg streptomycin ml–1 (the lowest concentrations tested). Strain DPN7T was able to grow slowly on agar plates containing ampicillin at concentrations up to the standard concentration for E. coli (75 µg ml–1).
To determine the sequence of the 16S rRNA gene, genomic DNA was extracted according to Marmur (1961). The gene was amplified by a PCR using Pfx DNA polymerase (MBI Fermentas) and total genomic DNA as template for the oligonucleotide primers 27f and 1525r, which were complementary to conserved regions of the 16S rRNA gene sequence of E. coli. The 1502 bp PCR product was purified using the NucleoTrap kit (Macherey-Nagel) and then sequenced. The PCR product was also ligated to EcoRV-linearized pBluescript II SK(–) (Stratagene) DNA and transformed into competent cells of E. coli TOP10. Plasmid DNA was isolated as described by Birnboim & Doly (1979).
DNA sequencing was performed by applying the SequiTherm long-read cycle sequencing kit (Epicenter Technologies), with the following oligonucleotides as sequencing primers: 27f (5'-GAGTTTGATCCTGGCTCAG-3'), 343r (5'-CTGCTGCCTCCCGTA-3'), 357f (5'-TACGGGAGGCAGCAG-3'), 519r [5'-G(T/A)-ATTACCGCGGC(T/G)GCTG-3'], 536f [5'-CAGC(C/A)GCCGCGGTAAT(T/A)C-3'], 803f (5'-ATTAGATACCCTGGTAG-3'), 907r (5'-CCGTCAATTCATTTGAGTTT-3'), 1114f (5'-GCAACGAGCGCAACCC-3'), 1385r [5'-CGGTGTGT(A/G)CAAGGCCC-3'] and 1525r (5'-AGAAAGGAGGTGATCCAGCC-3'), as well as the universal primer 5'-GTAAAACGACGGCCAGT-3' and the reverse primer 5'-CAGGAAACAGCTATGAC-3' that hybridize to pBluescript II SK(–). Sequence reactions were accomplished by using the GeneReadIR 4200 DNA analyser (LI-COR). 16S rRNA gene sequences were analysed using the program BLAST (National Center for Biotechnology Information; http://www.ncbi.nlm.nih.gov) by running the BLASTN program. The nucleotide sequence of the 16S rRNA gene of strain DPN7T and of related type strains belonging to the same phylogenetic group and also to well-known representatives of the Betaproteobacteria were aligned using CLUSTAL X (Thompson et al., 1997). 16S rRNA gene sequences were retrieved from the EMBL database and from the Ribosomal Database Project (Maidak et al., 1997). The resulting trees, displayed with TreeView (Page, 1996), were calculated by using the neighbour-joining method (Saitou & Nei, 1987).
The nucleotide sequence of the 16S rRNA gene of strain DPN7T shows high levels of sequence similarity (98.6–98.0 %) to several Alcaligenes sp. strains (Hiraishi et al., 2003; Boivin-Jahns et al., 1996), but these strains could not be analysed further since they are no longer available (R. Christen, personal communication). A sequence similarity of 98.5 % with respect to the type strain of the recently isolated and classified species Tetrathiobacter kashmirensis (Ghosh et al., 2005) was found, whereas lower similarity values were found with respect to the type strains of Castellaniella defragrans (strain 54PinT) (95.1 %), Alcaligenes faecalis (the type species of the genus Alcaligenes) (94.0 %), Alcaligenes latus (88.9 %) and Taylorella equigenitalis (94.7 %). The phylogenetic position of strain DPN7T is illustrated in a neighbour-joining dendrogram with Burkholderia kururiensis as the outgroup (Fig. 2).
|
, which were then separated by HPLC using a Waters Symmetry Shield C8 column thermostatted at 37 °C. The solvent used was 0.02 M NH4H2PO4 (pH 4.0) with 1.5 % acetonitrile. Non-methylated 
phage DNA (Sigma) was used as the calibration reference. The DNA G+C content of strain DPN7T was 55.1 mol%, which is the same as that reported for Tetrathiobacter kashmirensis LMG 22695T. The separated phylogenetic position of strain DPN7T was confirmed by DNA–DNA hybridization. Experiments were performed at 42 °C with photobiotin-labelled probes in microplate wells as described previously (Goris et al., 1998), using an HTS7000 Bio Assay Reader (PE Applied Biosystems) for the fluorescence measurements. The value for DNA–DNA hybridization to Tetrathiobacter kashmirensis LMG 22696 was only 41.4 %, whereas the values obtained with A. faecalis subsp. faecalis LMG 1229T and with C. defragrans LMG 18538T were low (7 and 5 %, respectively).
Agarose gel electrophoresis of crude extracts of cells of strain DPN7T obtained by the method of Birnboim & Doly (1979) revealed the presence of a 22 kbp plasmid. In preliminary experiments, this plasmid could not be connected with the capacity to utilize DTDP or other organic sulfur compounds. No plasmids were detected in Tetrathiobacter kashmirensis LMG 22695T or Tetrathiobacter kashmirensis LMG 22696.
Fatty acid analysis was carried out with a loopful of well-grown cells after an incubation period of 48 h. Fatty acid methyl esters were prepared, separated and identified using the Microbial Identification System (Microbial ID) as described previously (Vandamme et al., 1992). Strain DPN7T contained the following fatty acid components: 12 : 0 (4.5 %), 16 : 0 (18.2 %), 17 : 0 cyclo (4.8 %), 16 : 0 3-OH (3.3 %), 18 : 1
7c (26.5 %), 18 : 0 (2.1 %), 19 : 08c cyclo (2.6 %), summed feature 2 (13.3 %, comprising 12 : 0 ALDE, 16 : 1 iso I and/or 14 : 0 3-OH) and summed feature 3 (23.3 %, comprising 16 : 17c and/or iso-15 : 0 2-OH) (summed features are groups of two or three fatty acids that cannot be distinguished using the Microbial Identification System). Members of this phylogenetic lineage typically contain 14 : 0 3-OH and 16 : 17c; therefore, the peaks designated as summed features 2 and 3 probably corresponded to these fatty acids. A comparison with the fatty acid profile of Tetrathiobacter kashmirensis LMG 22695T (data available in Ghosh et al., 2005) revealed only small variations in composition.
The whole-cell protein profile of strain DPN7T was determined by using SDS-PAGE (Pot et al., 1994) and was compared with those of reference taxa belonging to this bacterial lineage. Data for reference strains were taken from previous studies (Coenye et al., 2003; Jang et al., 2001). The protein profile of strain DPN7T was clearly different from those of Alcaligenes, Achromobacter, Bordetella, Castellaniella and Taylorella reference strains, as well as from the type species of the genus Tetrathiobacter (Fig. 3).
|
) and complex media appeared to be identical. In addition, the DNA G+C contents of the two strains were the same (55.1 mol%), but the DNA–DNA hybridization value was relatively low (only 41.4 %); much lower values (7 and 5 %, respectively) were obtained with A. faecalis subsp. faecalis LMG 1229T and C. defragrans LMG 18538T. Furthermore, the physiological and biochemical characteristics of strain DPN7T (Table 1
), particularly with regard to utilization of the organic disulfide DTDP, led to the phylogenetic differentiation of strain DPN7T and Tetrathiobacter kashmirensis. Therefore, strain DPN7T should be classified as the type strain of a novel species of the genus Tetrathiobacter, for which the name Tetrathiobacter mimigardefordensis sp. nov. is proposed.
Description of Tetrathiobacter mimigardefordensis sp. nov.
Tetrathiobacter mimigardefordensis (mi.mi.gar.de.for.den'sis. M.L. masc. adj. mimigardefordensis of Mimegardefordum, a medieval name of Münster, where the type strain was isolated).
Cells are motile, Gram-negative, non-spore-forming coccoid rods (approx. 1.5–2 µm in length). They are oxidase- and catalase-positive, showing an oxidative metabolism. The temperature range for growth is 15–40 °C and the best growth occurs at 30–37 °C. Colonies on DTDP-containing agar plates are more flat than convex, up to 3 mm in diameter and white to lime-yellowish in colour, showing an increase in yellow colour with culture age. On complex medium, colonies grow in 1–2 days and appear more white than yellow and are up to 5 mm in diameter. Susceptible to kanamycin, gentamicin, tetracycline and streptomycin, with no significant antibiotic resistance. Fatty acid profile largely comprises 18 : 17c (26.5 %), 16 : 0 (18.2 %) and of the two fatty acids 16 : 17c and/or iso-15 : 0 2-OH (together constituting 23.3 %), which cannot be distinguished using the Microbial Identification System. The DNA G+C content of the type strain is 55.1 mol%. Carbon sources utilized are indicated in Table 1.
The type strain, DPN7T (=DSM 17166T=LMG 22922T), was isolated from a sample of matured compost from the compost plant in Münster (Germany).
|
ACKNOWLEDGEMENTS |
|---|
|
REFERENCES |
|---|
|
TOPABSTRACTMAIN TEXTREFERENCES |
|---|
Blenden, D. C. & Goldberg, H. S. (1964). Silver impregnation stain for Leptospira and Flagella. J Bacteriol 89, 899–900.
Boivin-Jahns, V., Ruimy, R., Bianchi, A., Daumas, S. & Christen, R. (1996). Bacterial diversity in a deep-subsurface clay environment. Appl Environ Microbiol 62, 3405–3412.[Abstract]
Brandl, H., Gross, A., Lenz, R. W. & Fuller, R. C. (1988). Pseudomonas oleovorans as a source of poly(-hydroxyalkanoates) for potential applications as biodegradable polyesters. Appl Environ Microbiol 54, 1977–1982.
Coenye, T., Vancanneyt, M., Falsen, E., Swings, J. & Vandamme, P. (2003). Achromobacter insolitus sp. nov. and Achromobacter spanius sp. nov., from human clinical samples. Int J Syst Evol Microbiol 53, 1819–1824.
Gerhardt, P., Murray, R. G. E., Wood, W. A. & Krieg, N. R. (editors) (1994). Methods for General and Molecular Bacteriology. Washington, DC: American Society for Microbiology.
Ghosh, W., Bagchi, A., Manda, S., Dam, B. & Roy, P. (2005). Tetrathiobacter kashmirensis gen. nov., sp. nov., a novel mesophilic, neutrophilic, tetrathionate-oxidizing, facultatively chemolithotrophic betaproteobacterium isolated from soil from a temperate orchard in Jammu and Kashmir, India. Int J Syst Evol Microbiol 55, 1779–1787.
Goris, J., Suzuki, K., De Vos, P., Nakase, T. & Kersters, K. (1998). Evaluation of a microplate DNA-DNA hybridization method compared with the initial renaturation method. Can J Microbiol 44, 1148–1153.[CrossRef]
Hiraishi, A., Narihiro, T. & Yamanaka, Y. (2003). Microbial community dynamics during start-up operation of flowerpot-using fed-batch reactors for composting of household biowaste. Environ Microbiol 5, 765–776.[CrossRef][Medline]
Jang, S. S., Donahue, J. M., Arata, A. B., Goris, J., Hansen, L. M., Earley, D. L., Vandamme, P. A. R., Timoney, P. J. & Hirsh, D. C. (2001). Taylorella asinigenitalis sp. nov., a bacterium isolated from the genital tract of male donkeys (Equus asinus). Int J Syst Evol Microbiol 51, 971–976.[Abstract]
Kertesz, M. A. (2000). Riding the sulfur cycle – metabolism of sulfonates and sulfate esters in Gram-negative bacteria. FEMS Microbiol Rev 24, 135–175.[Medline]
Kiene, R. P., Linn, L. J. & Bruton, J. A. (2000). New and important roles for DMSP in marine microbial communities. J Sea Res 43, 209–224.[CrossRef]
Lomans, B. P., van der Drift, C., Pol, A. & Op den Camp, H. J. M. (2002). Microbial cycling of volatile organic sulfur compounds. Cell Mol Life Sci 59, 575–588.[CrossRef][Medline]
Lütke-Eversloh, T. & Steinbüchel, A. (2003). Novel precursor substrates for polythioesters (PTE) and limits of PTE biosynthesis in Ralstonia eutropha. FEMS Microbiol Lett 221, 191–196.[CrossRef][Medline]
Lütke-Eversloh, T. & Steinbüchel, A. (2004). Microbial polythioesters. Macromol Biosci 4, 165–174.[CrossRef]
Lütke-Eversloh, T., Bergander, K., Luftmann, H. & Steinbüchel, A. (2001a). Identification of a new class of biopolymer: bacterial synthesis of sulfur-containing polymer with thioester linkages. Microbiology 147, 11–19.
Lütke-Eversloh, T., Bergander, K., Luftmann, H. & Steinbüchel, A. (2001b). Biosynthesis of poly(3-hydroxybutyrate-co-3-mercaptobutyrate) as a sulfur analogue to poly(3-hydroxybutyrate) (PHB). Biomacromolecules 2, 1061–1065.[CrossRef][Medline]
Lütke-Eversloh, T., Fischer, A., Remminghorst, U., & 8 other authors (2002). Biosynthesis of novel thermoplastic polythioesters by engineered Escherichia coli. Nat Mater 1, 236–240.[CrossRef][Medline]
Maidak, B. L., Olsen, G. J., Larsen, N., Overbeek, R., McCaughey, M. J. & Woese, C. R. (1997). The RDP (Ribosomal Database Project). Nucleic Acids Res 25, 109–111.
Marmur, J. (1961). A procedure for the isolation of desoxyribonucleic acid from microorganisms. J Mol Biol 1, 208–218.
McFarland, B. L. (1999). Biodesulfurization. Curr Opin Microbiol 2, 257–264.[CrossRef][Medline]
Mesbah, M., Premachandran, U. & Whitman, W. B. (1989). Precise measurement of the G+C content of deoxyribonucleic acid by high-performance liquid chromatography. Int J Syst Bacteriol 39, 159–167.
Mohn, W. W. (1995). Bacteria obtained from a sequencing batch reactor that are capable of growth on dehydroabietic acid. Appl Environ Microbiol 61, 2145–2150.[Abstract]
Mukhopadhyaya, P. N., Deb, C., Lahiri, C. & Roy, P. (2000). A soxA gene, encoding a diheme cytochrome c, and sox locus, essential for sulfur oxidation in a new sulfur lithotrophic bacterium. J Bacteriol 182, 4278–4287.
Page, R. D. M. (1996). TreeView: an application to display phylogenetic trees on personal computers. Comput Appl Biosci 12, 357–358.
Pedr
s-Alio, C., Mas, J. & Guerrero, R. (1985). The influence of poly--hydroxybutyrate accumulation on cell volume and buoyant density in Alcaligenes eutrophus. Arch Microbiol 143, 178–184.[CrossRef]
Pot, B., Vandamme, P. & Kersters, K. (1994). Analysis of electrophoretic whole-organism protein fingerprints. In Chemical Methods in Prokaryotic Systematics, pp. 493–521. Edited by M. Goodfellow & A. G. O'Donnell. Chichester: Wiley.
Saitou, N. & Nei, M. (1987). The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol Biol Evol 4, 406–425.[Abstract]
Sambrook, J., Fritsch, E. F. & Maniatis, T. (1989). Molecular Cloning: a Laboratory Manual, 2nd edn. Cold Spring Harbor, NY: Cold Spring Harbor Laboratory.
Schlegel, H. G., Kaltwasser, H. & Gottschalk, G. (1961). A submersion method for culture of hydrogen-oxidizing bacteria: growth physiological studies. Arch Mikrobiol 38, 209–222 (in German).[CrossRef][Medline]
Thompson, J. D., Gibson, T. J., Plewniak, F., Jeanmougin, F. & Higgins, D. G. (1997). The CLUSTAL_X windows interface: flexible strategies for multiple sequence alignment aided by quality analysis tools. Nucleic Acids Res 25, 4876–4882.
Timm, A., Byrom, D. & Steinbüchel, A. (1990). Formation of blends of various poly(3-hydroxyalkanoic acids) by a recombinant strain of Pseudomonas oleovorans. Appl Microbiol Biotechnol 33, 296–301.[CrossRef]
Vandamme, P., Vancanneyt, M., Pot, B. & 10 other authors (1992). Polyphasic taxonomic study of the emended genus Arcobacter with Arcobacter butzleri comb. nov. and Arcobacter skirrowii sp. nov., an aerotolerant bacterium isolated from veterinary specimens. Int J Syst Bacteriol 42, 344–356.
Van Hamme, J. D., Fedorak, P. M., Foght, J. M., Gray, M. R. & Dettman, H. D. (2004). Use of a novel fluorinated organosulfur compound to isolate bacteria capable of carbon–sulfur bond cleavage. Appl Environ Microbiol 70, 1487–1493.
Yoch, D. C. (2002). Dimethylsulfoniopropionate: its sources, role in the marine food web, and biological degradation to dimethylsulfide. Appl Environ Microbiol 68, 5804–5815.
This article has been cited by other articles:
|
|
 |
|
  N. Bruland, S. Bathe, A. Willems, and A. Steinbuchel Pseudorhodoferax soli gen. nov., sp. nov. and Pseudorhodoferax caeni sp. nov., two members of the class Betaproteobacteria belonging to the family Comamonadaceae Int J Syst Evol Microbiol, November 1, 2009; 59(11): 2702 - 2707. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
A. Gibello, A. I. Vela, M. Martin, A. Barra-Caracciolo, P. Grenni, and J. F. Fernandez-Garayzabal Reclassification of the members of the genus Tetrathiobacter Ghosh et al. 2005 to the genus Advenella Coenye et al. 2005 Int J Syst Evol Microbiol, August 1, 2009; 59(8): 1914 - 1918. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 B. Dam, W. Ghosh, and S. K. Das Gupta Conjugative Type 4 Secretion System of a Novel Large Plasmid from the Chemoautotroph Tetrathiobacter kashmirensis and Construction of Shuttle Vectors for Alcaligenaceae Appl. Envir. Microbiol., July 1, 2009; 75(13): 4362 - 4373. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
J. H. Wubbeler, N. Bruland, K. Kretschmer, and A. Steinbuchel Novel Pathway for Catabolism of the Organic Sulfur Compound 3,3'-Dithiodipropionic Acid via 3-Mercaptopropionic Acid and 3-Sulfinopropionic Acid to Propionyl-Coenzyme A by the Aerobic Bacterium Tetrathiobacter mimigardefordensis Strain DPN7 Appl. Envir. Microbiol., July 1, 2008; 74(13): 4028 - 4035. [Abstract] [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
| INT J SYST EVOL MICROBIOL | MICROBIOLOGY | J GEN VIROL |
| J MED MICROBIOL | ALL SGM JOURNALS | |
