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Applied and Environmental Microbiology, October 1998, p. 3824-3830, Vol. 64, No. 10
Department of Animal
Science1 and
Section of
Microbiology,2 Cornell University, Ithaca,
New York 14853
Received 22 December 1997/Accepted 14 July 1998
The 16S rRNA sequences and selected phenotypic characteristics were
determined for six recently isolated bacteria that can tolerate high
levels of hydrolyzable and condensed tannins. Bacteria were isolated
from the ruminal contents of animals in different geographic locations,
including Sardinian sheep (Ovis aries), Honduran and
Colombian goats (Capra hircus), white-tail deer
(Odocoileus virginianus) from upstate New York, and Rocky
Mountain elk (Cervus elaphus nelsoni) from Oregon. Nearly
complete sequences of the small-subunit rRNA genes, which were obtained
by PCR amplification, cloning, and sequencing, were used for
phylogenetic characterization. Comparisons of the 16S rRNA of the six
isolates showed that four of the isolates were members of the genus
Streptococcus and were most closely related to ruminal
strains of Streptococcus bovis and the recently described
organism Streptococcus gallolyticus. One of the other
isolates, a gram-positive rod, clustered with the clostridia in
the low-G+C-content group of gram-positive bacteria. The sixth isolate,
a gram-negative rod, was a member of the family Enterobacteriaceae in the gamma subdivision of the class
Proteobacteria. None of the 16S rRNA sequences of the
tannin-tolerant bacteria examined was identical to the sequence of any
previously described microorganism or to the sequence of any of the
other organisms examined in this study. Three phylogenetically distinct
groups of ruminal bacteria were isolated from four species of ruminants in Europe, North America, and South America. The presence of
tannin-tolerant bacteria is not restricted by climate, geography, or
host animal, although attempts to isolate tannin-tolerant bacteria from
cows on low-tannin diets failed.
The toxicity of phenolic compounds
in the environment has fostered studies of bacteria that are able
to tolerate and/or metabolize high levels of these compounds,
particularly under anaerobic conditions (1, 4, 14, 21, 30,
36). Tannins are secondary polyphenolic compounds known primarily
for their ability to bind to and precipitate proteins and other
macromolecules. Tannins have been found in many habitats, including
sewage sludge, forest litter, and the rumen (9, 14, 15, 28).
Bacteria capable of degrading or tolerating tannins have been isolated
from sewage sludge (14) and from the alimentary tracts
of koalas (Phascolarctos cinereus) (33), goats
(Capra hircus) (4, 30), and horses
(Equus caballus) (31). Most of the isolates have
been characterized phenotypically, and phylogenetic characterization
has been limited to studies conducted in Australia (4, 34,
35) and Japan (31). Little is known about the
geographic diversity and host species diversity of tannin-tolerant and
tannin-degrading bacteria.
The objective of this study was to characterize six recently isolated
tannin-tolerant bacteria by examining their phenotypic characteristics
and molecular phylogeny. These bacteria were isolated from the ruminal
contents of goats (C. hircus), sheep (Ovis
aries), white-tail deer (Odocoileus virginianus), and
Rocky Mountain elk (Cervus elaphus nelsoni), all of
which had consumed forage containing tannins. Our goal was to
genetically and biochemically characterize tannin-tolerant bacteria
isolated from different host animals in various geographic
locations.
Chemicals.
Tannic acid, p-coumaric acid, ferulic
acid, gallic acid, pyrogallol, and phloroglucinol were purchased from
Sigma Chemical Company, St. Louis, Mo. Quebracho tannin is an extract
of Schinopsis balansae and is commonly used as a standard
compound in tannin assays (19). Spray-dried quebracho was
purchased from Trask Chemical Company, Marietta, Ga. Desmodium
(Desmodium ovalifolium) is a tropical forage legume which
may contain more than 29% condensed tannin on a dry matter basis
(17). Lyophilized desmodium was obtained from Honduras, and
freeze-dried myrtle (Mirtus communis), a browse species from
the Mediterranean region, was obtained from Sardinia. The reagents
used, including acetic, propionic, and butyric acids, were analytical
grade.
Condensed tannin purification.
Condensed tannins were
purified with Sephadex LH-20 by using the method of Asquith and Butler
(2), as modified by Hagerman and Butler (20).
Culture technique and media.
The anaerobic culture
techniques of Hungate (22), with modifications
(5), were used for all incubations. Rum 10 medium (26) was used for initial transfers of ruminal fluid from
foreign animals before isolation of the tannin-tolerant bacteria.
Ruminal fluid medium (6), which was used for all incubations
except those in which the ability to utilize or tolerate different
substrates was tested, contained 0.3% (wt/vol) glucose as the carbon
source. Filter-sterilized carbohydrates were added after autoclaving. Ruminal fluid for the medium was obtained from a nonlactating cow fed
medium-quality grass hay without tannins. The ruminal fluid was
clarified aerobically by centrifugation at 20,000 × g
for 20 min at 4°C.
0099-2240/98/$04.00+0
Copyright © 1998, American Society for Microbiology. All rights reserved.
Phenotypic and Phylogenetic Characterization of
Ruminal Tannin-Tolerant Bacteria
ABSTRACT
Top
Abstract
Introduction
Materials & Methods
Results
Discussion
References
INTRODUCTION
Top
Abstract
Introduction
Materials & Methods
Results
Discussion
References
MATERIALS AND METHODS
Top
Abstract
Introduction
Materials & Methods
Results
Discussion
References
Isolation of bacteria. Attempts were made to isolate bacteria from five species of ruminants in five different geographical locations, including Sardinian sheep, Honduran goats, Colombian goats, Rocky Mountain elk from Oregon, and domesticated cattle and white-tail deer from upstate New York. All of the animals except the cattle had consumed material containing tannins. The goats in Honduras and Colombia had been fed diets containing a tropical forage legume (Desmodium spp.), and the Sardinian sheep had been fed diets containing myrtle. White-tail deer in New York are known to consume oak (Quercus spp.), red maple (Acer rhubrum), and sugar maple (Acer saccharum) in the late fall. The Rocky Mountain elk in Oregon had been fed diets that contained fireweed (Epilobium angustifolium), red osier dogwood (Cornus stolonifera), Rocky Mountain maple (Acer glabrum), and alder (Alnus incana) (42). The cattle were fed predominantly grass hay and had never consumed feeds containing high levels of tannins.
Ruminal fluid was collected from sheep and goats orally with stomach tubes. Rocky Mountain elk ruminal contents were obtained with a stomach tube after the animals had been anesthetized, and samples of white-tail deer digesta were obtained from animals slaughtered during hunting season. Ruminal fluid from nonlactating Holstein cows was collected through fistulas. Ruminal fluid from foreign animals was transferred twice in Rum 10 medium immediately after it was collected and prior to inoculation into ruminal fluid medium containing either tannic acid or quebracho at a concentration of 1 g/liter. The two successive transfers were necessary to meet importation requirements. Sardinian, Colombian, and Honduran samples were hand carried to Cornell University and arrived within 24 h of shipment. The elk ruminal fluid from Oregon was strained through cheesecloth and then inoculated directly into ruminal fluid medium containing either tannic acid or quebracho. Samples were shipped by overnight delivery and arrived within 24 h of collection. The elk samples were immediately frozen in a 20% glycerol solution and stored at
80°C. These samples were later thawed for culturing.
The white-tail deer samples were hand carried in a thermos purged with
oxygen-free CO2 immediately following slaughter of the
animals. The samples were immediately strained through cheesecloth
before being subcultured. Aliquots of the deer ruminal fluid were
inoculated into enrichment medium within 6 h of collection.
Upon arrival at our laboratory, the ruminal bacteria from goats, sheep,
and white-tail deer were subcultured three times with 2-day intervals
between transfers in ruminal fluid medium containing either 1 g of
tannic acid per liter or 1 g of quebracho per liter. The Rocky
Mountain elk samples were thawed anaerobically before being
subcultured. After the initial transfer, cultures were plated on
ruminal fluid medium (6) containing 3% (wt/vol) agar and then were overlaid with 2 ml of a 10% (wt/vol) tannic acid solution or
2 ml of a 10% (wt/vol) purified quebracho solution. An anaerobic chamber (Coy, Ann Arbor, Mich.) with an atmosphere containing 94%
CO2 and 6% H2 was used for plating
experiments. Isolated colonies were selected and inoculated into
ruminal fluid broth medium containing tannic acid or unpurified
quebracho at a concentration of 1 g/liter. Weekly transfers were
necessary for survival of the cultures. For long-term storage, cultures
were frozen in 20% glycerol and stored at 80°C.
The cell wall types of the strains isolated were determined by the Gram
stain method. Cultures for which the Gram stain results were variable
were tested for monensin susceptibility as previously described
(40). Cell size was measured during the mid-exponential phase of growth by phase-contrast microscopy by using a confocal scanning microscope.
Growth studies. For all growth studies, 0.3-ml portions of mid-exponential-phase cultures grown in ruminal fluid medium were inoculated into 9.7-ml portions of the appropriate medium. The isolates were tested for the ability to utilize ammonium chloride, amino acids, and casein as nitrogen sources and the ability to use different carbohydrates as energy sources. Carbohydrate fermentation characteristics and enzymatic activities were determined for the gram-negative rod-shaped organism strain KN4 with an API 20E commercial identification kit (API System, Montalieu Vercieu, France).
The ability to utilize hydrolyzable and condensed tannins and phenolic monomers as sole energy sources and the ability to tolerate these compounds in the presence of supplemental carbohydrates were evaluated. Responses to oxygen also were tested under aerobic and microaerophilic conditions. To study the tolerance of the bacteria to different phenolic compounds, cultures were inoculated into defined medium (8) lacking glucose (negative control), defined medium containing glucose (positive control), and defined medium containing glucose and the compound of interest (phenolic monomer, tannic acid, unpurified quebracho, or desmodium that had been purified with Sephadex LH-20 [2], as modified by Hagerman and Butler [20]). Tolerance was assessed by determining the maximum concentration of added phenolic compound at which there was growth, as measured by a change in absorbance at 600 nm (A600) when cultures were compared with the appropriate blank. The phenolic monomers tested included p-coumaric acid, ferulic acid, gallic acid, pyrogallol, and phloroglucinol. After they were dissolved in phosphate buffer (pH 6.8) (18), the phenolic monomers were filter sterilized and added to the medium at final concentrations of 1, 5, 10, 20, 30, 40, and 50 mM. Tannic acid, unpurified quebracho, and purified desmodium were added at concentrations of 1.0, 2.0, 2.5, 3.0, 3.5, 4.0, 8.0, and 10.0 g/liter. The effect on the growth rate was monitored by measuring changes in the A600 caused by bacterial growth compared with the A600 of a blank containing medium and the appropriate concentration of the phenolic compound being tested. Values were obtained with a Spectronic 601 spectrophotometer (Milton Roy, Rochester, N.Y.). To determine the volatile fatty acid and lactate production profiles of isolated cultures, 1.5-ml aliquots of the culture medium were centrifuged at 4,000 × g for 5 min, and the supernatant was removed. A 360-µl aliquot of each sample was transferred to a microcentrifuge tube containing 40 µl of 50 mM H2SO4. After the tube contents were mixed and allowed to stand at room temperature for 10 min, each preparation was centrifuged again, and the supernatant was analyzed to determine the volatile fatty acid content by the high-pressure liquid chromatography method of Ehrlich et al. (11). A mixture of acetic, propionic, isobutyric, butyric, fumaric, and lactic acids was used as a calibration standard in all analyses. To measure tannic acid degradation, cultures were grown in the presence of tannic acid at a concentration of 1 g/liter. At the end of each fermentation, 1-ml aliquots of culture medium were mixed with 50-mg portions of polyvinylpyrrolidone (PVP) to remove the residual tannic acid. Samples were incubated at room temperature for 60 min to permit PVP-tannin binding and then were centrifuged at 6,000 × g for 10 min. The affinity of phenolic monomers to PVP is low because of the limited number of hydroxyl groups available for binding (10). As a result, the breakdown products resulting from tannic acid degradation remained in the supernatants. One-milliliter aliquots of each supernatant were analyzed to determine the total phenolic compound content by using the Prussian blue method of Price and Butler (38), which quantified the concentration of phenolic hydroxyl groups in the sample but did not provide structural information on the phenolic compounds. The presence of pyrogallol, phloroglucinol, and gallate was determined by gas chromatography-mass spectrometry. To detect pyrogallol, phloroglucinol, or gallate, trimethylsilyl derivatives were prepared and analyzed with a Hewlett-Packard model 5890 series 2 gas chromatograph. Isolated phenolic end products and nonvolatile components were prepared by extracting the supernatant from cells grown with the compounds in an equal volume of ethyl acetate and drying the extracts under CO2. Compounds were separated on an HP-5 column cross-linked with 5% phenyl methyl siloxane; the column was 30 cm long, had an internal diameter of 0.25 mm and a film thickness of 0.25 µm, and was obtained from Hewlett-Packard Co., Wilmington, Del. The temperature gradient used was 40 to 250°C. Chromatographic peaks were identified by comparison with a gas chromatography-mass spectrometry internal library or with authentic samples. Degradation of hydrolyzable tannin-protein complexes was evaluated by a modification of the method of Osawa (32). The formation of zones of clearing when the bacteria were grown anaerobically on brain heart infusion agar plates (Difco Laboratories) which had been overlaid with 2 ml of a 10% (wt/vol) tannic acid solution was monitored. All of the isolates were tested simultaneously.Extraction of DNA and amplification and cloning of the 16S rRNA genes. Zirconium-silica beads (0.8 g of 0.1-mm-diameter beads) were added to 800-µl portions of cultures in the late-exponential phase of growth. The cells were disrupted with a Mini-BeadBeater-8 (Biospec Products Inc., Bartlesville, Okla.) for 3 min. Total DNA was extracted from each lysate with an equal volume of phenol-chloroform-isoamyl alcohol (50:49:1) (3). The DNA was resuspended in double-distilled water to the original volume (800 µl) and was used for the subsequent PCR.
The 16S rRNA gene was amplified by PCR (23) with a forward primer corresponding to nucleotide positions 8 to 27 of Escherichia coli 16S rRNA (24) (forward primer 8FPL; 5'-CGGATCCGCGCCGCTGCAGAGTTTGATCCTGGCTCAG-3') and a primer corresponding to the reverse complement of positions 1510 to 1492 (reverse primer 1492RPL; 5'-GGCTCGAGCGGCCGCCCGGGTTACCTTGTTACGACTT-3'). Primer 8FPL is specific for members of the domain Bacteria, whereas 1492RPL is a universal primer and aligns with sequences conserved in all three phylogenetic domains (39). Each 50-µl reaction mixture contained each primer at a concentration of 0.1 µM, 0.2 mM dCTP, 0.2 mM dATP, 0.2 mM dGTP, 0.2 mM dTTP, 5 µl of a 10× Gibco PCR buffer (200 mM Tris-HCl [pH 8.4], 500 mM KCl) (Life Technologies, Grand Island, N.Y.), 2.5 U of Gibco Taq DNA polymerase, 3 mM MgCl2, and 5 µl of resuspended bacterial DNA, which corresponded to approximately 106 DNA molecules (23). Each amplification mixture was overlaid with mineral oil before it was incubated in an Amplitron II thermal cycler (Thermolyne, Dubuque, Iowa). The program consisted of 30 cycles consisting of denaturation at 94°C for 30 s, annealing at 55°C for 30 s, and extension at 72°C for 1 min. There was a 5-min denaturation step at 94°C before the first cycle, and there was a 5-min extension step at 72°C after the 30th cycle. For each set of PCR, negative controls that contained no added template were included. Amplified DNA for cloning was electrophoresed and extracted from a 1.5% agarose gel by using a Qiaex II gel extraction kit (Qiagen, Hilden, Germany). The extracted DNA fragments were cloned into PCR 2.1 (Invitrogen, San Diego, Calif.). About 15 clones from each ligation transformation reaction were selected. Because each of the clones from the same ligation had the same insert size based on ligation product digests, one clone was selected for sequencing. Plasmid DNA was extracted by using the Wizard Minipreps DNA purification system (Promega). Extracts were prepared for sequencing by gel purification by using a BstEII digest of lambda DNA (US Biochemical Corporation, Cleveland, Ohio) as a molecular weight standard. The purified plasmid preparations were sequenced directly with an ABI automated DNA sequencer by using a Prism dideoxy terminator cycle sequencing kit and the recommended sequencing protocol (Perkin-Elmer, Foster City, Calif.). Forward and reverse DNA-specific primers, as well as internal primers, were used for sequencing. The internal sequencing primers used to obtain the complete 16S ribosomal DNA sequences were P520 (5'-CAGCAGCCGCGGTAATAC; positions 520 to 537) and P1090 (5'-TTAAGTCCCGCAACGAGCG; positions 1090 to 1108).Phylogenetic analyses. Phylogenetic analyses were performed by using the PHYLIP phylogeny inference package, version 3.5c (12, 13). In the initial analysis, the sequences obtained were compared with the 16S rRNA sequences of organisms in the domain Bacteria obtained from the Ribosomal Database Project (RDP) (27) by using the SUGGEST TREE function. Aligned sequences of the resulting closest relatives and other sequences known to belong to the same phylogenetic group were retrieved from the RDP library. Our 16S rRNA sequences were manually aligned with these retrieved sequences.
Pairwise evolutionary distances were computed from the aligned sequences by using the PHYLIP program (12), DNADIST, and a Kimura model for nucleotide substitution, and trees were generated by using NEIGHBOR. The stability associated with treeing orders was evaluated by using the programs SEQBOOT, DNADIST, NEIGHBOR, and CONSENSE within the PHYLIP program. One hundred bootstrap trees were generated for each dataset.Nucleotide sequence accession numbers. The designations and GenBank accession numbers of the bacteria used in the phylogenetic analyses are listed below. The accession numbers of the bacteria used in the analysis of the streptococci (Fig. 1) were ATCC 43077, ATCC 27823, ATCC 27335, ATCC 33317, NCDO 597, ACM 3969, ATCC 19642, ATCC 33748, ATCC 9812, X94337, ATCC 35911, NCTC 3165, ATCC 25175, ATCC 19615, ATCC 19645, ATCC 15300, ATCC 33478, ATCC 27958, and NCDO 2156.
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RESULTS |
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Top
Abstract
Introduction
Materials & Methods
Results
Discussion
References
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Physiological characteristics. When ruminal contents were plated onto agar overlaid with tannic acid, we were able to isolate colonies from digesta of all of the animals except the cows at Cornell University. Despite repeated attempts at enrichment and isolation, we were unable to isolate tannin-tolerant bacteria from the cows, which had no history of tannin consumption. Six tannin-tolerant colonies, two each from goats and elk and one each from sheep and deer, were selected for further characterization. None of these bacteria was able to grow in medium containing condensed tannins as the sole carbon source. Based on phylogenetic and phenotypic characterization, the bacteria fell into three groups, which are discussed below.
Strains KN1, KN2, KN3, and TW1 were gram-positive cocci that were isolated from the ruminal contents of a goat in Colombia, a goat in Honduras, a sheep in Sardinia, and a Rocky Mountain elk in the United States, respectively. The isolate from the Colombian goat, KN1, was described elsewhere recently (30). A gram-negative rod-shaped organism, strain KN4, was isolated from the ruminal contents of a white-tail deer from upstate New York, and strain TW2 is a gram-positive rod-shaped organism that was isolated from Rocky Mountain elk ruminal contents in Oregon (Table 1). Some of the physiological and biochemical characteristics of the isolates are shown in Tables 1 and 2. All of the isolates were able to utilize ammonia, amino acids, or casein as a sole N source and grew on glucose, lactose, galactose, or cellobiose as a carbon source.
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-galactosidase, arginine dihydrolase, and lysine
decarboxylase activities but was not able to hydrolyze urea,
did not produce hydrogen sulfide, and did not have tryptophan deaminase
or oxidase activity. It could utilize sorbitol, rhamnose, and melibiose
but not citrate, gelatin, inositol, saccharose, or amygdalin.
The gram-positive, rod-shaped organism TW2 was a strict anaerobe.
Endospores were not detected microscopically, and no growth occurred
after incubation at 80°C for 10 min. This bacterium utilized a
variety of sugars and was capable of degrading cellulose. This isolate
produced lactate, acetate, and butyrate as fermentation products.
Phylogenetic analysis of the 16S rRNA sequences. The use of primers which corresponded to more than one conserved region allowed us to generate nearly complete 16S rRNA sequences for the six isolates (24). The sequences corresponded to positions 28 to 1491 of the E. coli 16S rRNA sequence. When the four gram-positive cocci were compared to representatives of the Bacteria included in the RDP database library, they formed a distinct cluster within the genus Streptococcus of the lactic acid bacteria and were most closely related to the recent ruminal isolates Streptococcus caprinus (4) and Streptococcus gallolyticus (34). The intercluster identity values for the 16S rRNA sequences of these four tannin-tolerant cocci ranged from 94 to 97%. The phylogenetic gene tree which resulted from our multiple-sequence analysis is shown in Fig. 1.
The gram-positive Rocky Mountain elk isolate (TW2) is a previously undescribed member of the genus Eubacterium. Figure 3 is a phylogenetic tree showing the evolutionary distances between this isolate and some other low-G+C-content gram-positive bacteria. Based on the phylogenetic classification of Collins et al. (7), TW2 is a member of subcluster XIVa, the subcluster that contains its closest relative, Eubacterium cellulosolvens, which also is cellulolytic.
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subdivision of the class Proteobacteria in the domain
Bacteria. Of the organisms in the RDP database, it was most
closely related to, but was not identical to, several strains of
E. coli.
Similarities to other tannin-tolerant and tannin-protein complex-degrading bacteria. None of the six isolates exhibited 100% rRNA sequence similarity with any available 16S rRNA gene sequence. The highest levels of similarity were between the gram-positive bacteria and their closest relatives, S. caprinus and S. gallolyticus. S. caprinus is a tannin-tolerant bacterium that was isolated from the ruminal contents of a feral goat (4). Recent comparisons have revealed that S. caprinus 2.3 is the same organism as S. gallolyticus, which was isolated from several species of animals, including koalas, pigs, horses, and dogs (41). All of the S. gallolyticus isolates that have been characterized have gallate decarboxylase activity. As S. gallolyticus was isolated before S. caprinus, the name S. gallolyticus has nomenclatural priority (41). We included both 16S rRNA sequences and names in our phylogenetic analyses. The four recent tannin-tolerant isolates obtained in our study clustered near S. gallolyticus and S. caprinus.
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DISCUSSION |
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Top
Abstract
Introduction
Materials & Methods
Results
Discussion
References
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Sequencing of the 16S rDNA enabled us to compare the recently isolated tannin-tolerant bacteria with available bacterial sequences in the EMBL and RDP (27) databases. Four of the six isolates which were examined formed a tight cluster within the genus Streptococcus. The studies of S. gallolyticus and S. caprinus of Osawa et al. (34) and Brooker et al. (4) indicated that there is a group of streptococci that are able to tolerate hydrolyzable and condensed tannins, as well as phenolic monomers. Some members of this group which had diverse origins also have gallate decarboxylase and/or tannase activities.
Osawa et al. (34) and Brooker et al. (4) identified bacteria isolated in Australia and Japan. In the present study we examined ruminal contents from three continents, Europe, North America, and South America, and found that the ability of ruminal bacteria to tolerate and/or degrade tannins is widespread. The ruminal contents of domestic temperate cattle from Cornell University did not yield tannin-tolerant bacteria. This was most likely because the animals had not previously consumed material containing tannins. S. bovis JB1, a well-studied ruminal strain, was quite intolerant of tannins and other phenolic compounds (Table 2).
In addition to having similar phylogenetic positions, three of our four ruminal streptococci could ferment mannitol, as could 90% of the S. gallolyticus strains isolated by Osawa et al. (34). S. bovis JB1 was not able to ferment mannitol. Our streptococci, however, could tolerate much higher levels of tannins and other phenolic compounds than S. bovis JB1 but could not cleave tannin-protein complexes, as determined by the zone-clearing method described by Osawa et al. (34) (Table 2). Some of the other important differences between our isolates and the strains isolated in Australia were the inability of S. caprinus or S. gallolyticus to use ammonia as a sole source of nitrogen and the production of different fermentation products. Our isolates produced lactate, fumarate, and acetate predominantly, while S. caprinus and S. gallolyticus produced small amounts of acetate and ethanol in addition to lactate.
Based on the results of biochemical characterization with an API test kit, gram-negative isolate KN4 is a member of a subgroup of E. coli (subgroup 7144552). This subgroup is very heterogeneous, and its members are uncommon strains of E. coli. The phylogenetic analyses demonstrated that KN4 is nested among E. coli strains and therefore most likely is an E. coli strain. An isolate from the rumen of a white-tail deer, KN4 is phenotypically similar to tannin-protein complex-degrading enterobacteria isolated from the alimentary tracts of koalas and described by Nemoto et al. (31) and Osawa (33). Osawa's isolates were variable in size and included a mixture of short rods and long filamentous rods. These rods produced zones of clearing on tannin-protein complex plates but were not able to use ammonia as a sole nitrogen source. They also could not ferment mannitol. These isolates have not been characterized yet at the genotypic level, so our comparisons were limited to biochemical data.
Osawa (33) suggested that his enterobacteria were related to Enterobacter agglomerans (reclassified as Pantoea agglomerans [16]), which is a human pathogen isolated from plants and animals. The 16S rRNA sequence of P. agglomerans was not available so it could not be included in our phylogenetic comparisons, but phenotypic and genetic characterization of P. agglomerans (16) showed that it consists of several biogroups. In addition, there is an Erwinia-P. agglomerans complex with at least 10 relatedness groups, all of which have taxonomic problems. Although KN4 may constitute another relatedness group within the Erwinia-P. agglomerans complex, it is different from the type strain of P. agglomerans, which is negative for ornithine decarboxylase, arginine dihydrolase, and lysine decarboxylase and can grow on sucrose.
Gram-positive rod-shaped strain TW2, which was isolated from the ruminal contents of a Rocky Mountain elk, was closely related to E. cellulosolvens, a gram-positive cellulolytic rod (Fig. 3). E. cellulosolvens has been isolated from the ruminal contents of sheep and cows and the intestinal tract of a hog (25). Based on the phylogenetic reclassification proposed by Collins et al. (7), isolate TW2 is a member of the phenotypically diverse taxon subcluster XIVa, and, not surprisingly, its closest neighbor is cellulolytic.
In this study, we identified three phylogenetically distinct groups of ruminal bacteria which tolerate tannins and other phenolic compounds. Not only do these bacteria differ phylogenetically, but the tannin-tolerant enterobacteria and streptococci are the first groups of tannin-tolerant bacteria known to have members that occur in markedly different geographical locations. All of the tannin-tolerant bacteria described here were able to use both ammonia and amino acids as N sources, suggesting that tannin tolerance is not dependent on the form of N utilized. Climate, geography, and host animal do not seem to affect the ability of the bacteria to tolerate tannins. This was demonstrated by the streptococcal isolates described in this paper. These isolates are similar in both biochemical characteristics and 16S rRNA sequences, yet they were isolated from four different species of animals living in temperate and tropical climates on three continents. Our phylogenetic analysis suggested that our streptococci (KN1, KN2, KN3, and TW1, as well as S. caprinus and S. gallolyticus) and the ancestor of the S. bovis complex have a common ancestor (Fig. 1).
Examination of the genomes of tannin-tolerant isolates for the genes which confer tannin tolerance, complete evaluation of the structure of the proteins associated with tannin tolerance, and ecological studies which allow monitoring of these novel bacteria in their natural setting are the next logical steps in interpreting interactions between tannins and bacteria.
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ACKNOWLEDGMENTS |
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We thank Yueh-Tyng Chien, Grace Lee, and Dave Hinman for advice on experiments. John Cook, a wildlife research biologist at the National Council of the Paper Industry for Air and Stream Improvement, LaGrande, Oreg., generously let us use his elk and provided useful advice which enabled us to collect ruminal samples from the elk. We are grateful to Miguel Vélez and Antonio Flores (Pan American School for Agriculture, Tegucigalpa, Honduras), Antonello Cannas (University of Sassari, Sassari, Sardinia, Italy), E. John Pollak (Cornell University), and Carlos Lascano (C.I.A.T, Cali, Colombia) for providing ruminal fluid. The technical assistance and recommendations of James Van Ee and Carol Bayles at the Sequencing Facility of the New York Center for Advanced Technology at Cornell University were greatly appreciated.
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FOOTNOTES |
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* Corresponding author. Mailing address: Department of Animal Science, Morrison Hall, Cornell University, Ithaca, NY 14853. Phone: (607) 255-2876. Fax: (607) 255-9829. E-mail: AP19{at}cornell.edu.
Present address: The Institute for Genomic Research, Rockville, MD
20850.
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REFERENCES |
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Abstract
Introduction
Materials & Methods
Results
Discussion
References
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