Toxicity of unsaturated fatty acids to the biohydrogenating ruminal bacterium, Butyrivibrio fibrisolvens
© Maia et al; licensee BioMed Central Ltd. 2010
Received: 28 August 2009
Accepted: 18 February 2010
Published: 18 February 2010
Health-promoting polyunsaturated fatty acids (PUFA) are abundant in forages grazed by ruminants and in vegetable and fish oils used as dietary supplements, but only a small proportion of PUFA finds its way into meat and milk, because of biohydrogenation in the rumen. Butyrivibrio fibrisolvens plays a major role in this activity. The aim of this study was to investigate the mechanisms by which PUFA affect the growth of B. fibrisolvens, how PUFA are metabolized and the metabolic response to growth in the presence of PUFA.
Linoleic acid (LA; cis-9, cis-12-18:2) and α-linolenic acid (LNA; cis-9, cis-12, cis-15-18:3) increased the lag phase of B. fibrisolvens JW11, LNA having the greater effect. Growth was initiated only when the PUFA had been converted to vaccenic acid (VA; trans- 11-18:1). The major fish oil fatty acids, eicosapentaenoic acid (EPA; 20:5(n- 3)) and docosahexaenoic acid (DHA; 22:6(n- 3)), were not metabolized and prevented growth. Cellular integrity, as determined fluorimetrically by propidium iodide (PI) ingression, was affected as much by 18:1 fatty acids, including VA, as 18:2 fatty acids. The methyl esters of LNA, LA, EPA and DHA had no effect on growth or other measurements. The ATP pool decreased by 2/3 when LA was added to growing bacteria, whereas most acyl CoA pools decreased by >96%.
It was concluded that biohydrogenation occurs to enable B. fibrisolvens to survive the bacteriostatic effects of PUFA, and that the toxicity of PUFA is probably mediated via a metabolic effect rather than disruption of membrane integrity.
Unsaturated fatty acids, particularly α-linolenic acid (LNA; cis-9, cis-12, cis-15-18:3) and linoleic acid (LA; cis-9, cis-12-18:2), are abundant in grass and other ruminant feedstuffs, yet are present at low concentrations in meat and milk. Furthermore, tissue lipids of ruminants have been known for a long time to be more saturated than those of non-ruminants . As the consumption of saturated acids in dairy products and ruminant meats is often associated with an increased incidence of coronary heart disease in man , the transformation of unsaturated fatty acids to saturated fatty acids, or biohydrogenation, in ruminants presents a major human health issue. The biohydrogenation process has long been known to occur in the rumen as the result of microbial metabolic activity [3, 4]. Thus, if ruminal biohydrogenation of unsaturated fatty acids can be controlled, it may be possible to improve the healthiness of ruminant meats and milk by increasing their unsaturated fatty acids composition in general and the n-3 fatty acids in particular . One of the unsaturated fatty acids that appears most desirable is conjugated linoleic acid (CLA; cis-9, trans-11-18:2) because of its anticarcinogenic and other health-promoting properties [6, 7]. Major advances have been made in achieving the desired changes in fatty acid content of meat and milk experimentally, via dietary manipulation in ruminants, generally by adding oils containing unsaturated fatty acids to the diet [5, 8–10]. The inclusion of fish oil in particular seems to alter biohydrogenating activity in the rumen .
Butyrivibrio fibrisolvens was identified many years ago to undertake biohydrogenation of fatty acids  and to form CLA as intermediate in the process . Kim et al.  noted that LA inhibited growth of B. fibrisolvens A38, an effect that depended both on the concentration of LA and the growth status of the bacteria. Growing bacteria were more tolerant of LA. In a study of CLA production in different strains of B. fibrisolvens, Fukuda et al.  found that the most tolerant strain had the highest linoleate isomerase (forming CLA from LA) specific activity. Different members of the Butyrivibrio/Pseudobutyrivibrio phylogenetic grouping, all of which biohydrogenate PUFA, had different sensitivities to growth inhibition by LA, the most sensitive possessing the butyrate kinase rather than the acyl transferase mechanism of butyrate production . For reasons that were unclear, lactate exacerbated the toxicity of LA to Clostridium proteoclasticum, now renamed Butyrivibrio proteoclasticus. The aim of this work was to understand the nature of the toxic effects of PUFA on B. fibrisolvens JW11. Strain JW11 is located in the middle of the numerous B. fibrisolvens/Pseudobutyrivibrio cluster, members of which share the ability to form CLA and vaccenic acid (VA; trans-11-18:1) but which also lack the ability to biohydrogenate VA to stearic acid (SA; 18:0) . Understanding these effects could have important indirect implications for human health by enabling ruminal biohydrogenation of dietary PUFA to be manipulated in order to provide healthier ruminant-derived foods.
Fatty acid metabolism by B. fibrisolvens JW11
Comparative effects of fatty acids and methyl esters on growth and metabolism by B. fibrisolvens JW11
Effects of fatty acids and methyl esters (50 μg ml-1) on growth of, and metabolism of fatty acids by, Butyrivibrio fibrisolvens JW11 in M2 medium.
Free fatty acids
Lag phase (h)
End product at 72 h
Lag phase (h)
End product at 72 h
Influence of fatty acids on cell integrity of B. fibrisolvens JW11
Influence of LA on ATP and acyl CoA pools of B. fibrisolvens JW11
Influence of LA on acyl CoA pools of B. fibrisolvens JW11 20 min after inoculation into fresh medium.
Acyl CoA concentration
(pmol mg protein-1)
0.2 mg ml-1LA
B. fibrisolvens was originally described as a small, Gram-positive bacterium particularly prevalent in the rumen of grazing animals . Many strains are proteolytic and involved in fibre breakdown [19, 20]. B. fibrisolvens JW11 was originally isolated as a proteolytic strain . It has been many years since the importance of B. fibrisolvens in the process of PUFA reduction, or biohydrogenation, was first documented . Although other bacteria have been implicated , biohydrogenating activity is high among all members of what is now known to be an extensive Butyrivibrio phylogenetic tree . Indeed, in our experience, its activity is many times higher than in other species . 'Type B' bacteria, which complete the reduction of 18:1 isomers to SA, was identified as C. proteoclasticum, which has recently been renamed Butyrivibrio proteoclasticus. The pattern of metabolism of LA and LNA observed here, and the identity of the intermediates, follows the pathways established first by Kepler et al.  and confirmed later by others [24–26]. The observations linking growth and LA metabolism with B. fibrisolvens JW11 are consistent with those obtained with B. fibrisolvens A38  and B. fibrisolvens TH1 . What is novel about the present observations is that they clearly demonstrate that biohydrogenation is a detoxification process, necessary to escape from the bacteriostatic effects of PUFA. Indeed, they explain that the concentration-dependence of LA toxicity and its apparently lower toxicity in growing cultures, observed by Kim et al. , have to be considered in terms of time required by different biomass concentrations to hydrogenate, and thereby detoxify, different concentrations of fatty acids.
Henderson  examined the effects of fatty acids on ruminal bacteria. A Butyrivibrio sp. was generally most sensitive to fatty acids, but only saturated and monoenoic acids were included in the study. OA was much more toxic than the saturated fatty acids. Marounek et al.  found that C-12 and C-14 fatty acids were more toxic to ruminal and rabbit caecal bacteria than other chain lengths, but again the study was of saturated acids and oleic acid. In non-ruminal bacteria, LA and LNA were much more toxic than saturated or monoenoic acids . The present paper describes the effects of the more abundant poly- and monounsaturated fatty acids on B. fibrisolvens. The PUFA were found to be much more toxic than more saturated fatty acids.
The present experiments help to resolve the purpose of biohydrogenation in the ruminal bacteria that undertake this reductive metabolism. Our results provide support for the conclusions of Harfoot and Hazlewood, Kemp and Lander  and Kemp et al.  that biohydrogenation is a detoxification mechanism rather than a means of disposing of reducing power, as proposed earlier . The reductase which converts CLA to VA in B. fibrisolvens comprises 0.5% of the total cell protein , a very significant expenditure of cellular resources that signifies a vital function. It should be noted that, although more research emphasis is placed on its metabolism of LA because CLA is an intermediate, biohydrogenation is probably more important for B. fibrisolvens to survive high LNA concentrations, as LNA is more toxic than LA and is usually present at higher concentrations than LA in forages (e.g. ). Also to be noted is that CLA is almost as toxic as LA, as found before .
There are several possible reasons why unsaturated fatty acids are generally more toxic than saturated fatty acids. The double bonds alter the shape of the molecule, such that kinked unsaturated fatty acids disrupt the lipid bilayer structure . The finding that different PUFA isomers, such as LNA and γ-LNA, had different toxicity would be consistent with such an interpretation. However, it is not clear that the toxicity was necessarily a membrane effect. The free carboxyl group was necessary for growth inhibition to take place. Methyl esters, which might be expected to be sufficiently hydrophobic to be incorporated into a membrane just as efficiently as a free fatty acid, were non-toxic. They were metabolized in the same way as the free fatty acids, however, as they were hydrolysed by bacterial esterase activity. The free carboxyl group was also necessary for disruption of cell integrity, as measured by PI ingression. However, PI ingression was affected little by the number of double bonds in the fatty acid molecule, as detected by both fluorescence spectroscopy and flow cytometry, and could not explain why 18:3 fatty acids were more toxic to growth than 18:2 fatty acids, and especially why 18:1 was not toxic to growth. Furthermore, sodium lactate exacerbated growth inhibition by LA, in a similar manner to that observed with B. proteoclasticus, but had no similar effect on the influence of LA on cell integrity of B. fibrisolvens. A similar conclusion was reached by Maia et al.  when comparing the toxic effects of fatty acids on growth and cell integrity in different species of ruminal bacteria. Thus, although a toxic mechanism involving disruption of the extraordinarily thin cell envelope of B. fibrisolvens seems an attractive and logical possibility, the evidence suggests that the primary effect of PUFA lies elsewhere.
An alternative possibility is that the ready diffusion of the free fatty acid across the membrane causes chemiosmotic difficulties, perhaps uncoupling the proton-motive force , dissipating the membrane potential by facilitating ion leakage  or decoupling intramembrane pathways [38, 39]. While this remains a possibility, the different effects on acyl CoA and ATP pools on PUFA toxicity suggest a metabolic effect, specifically in acyl CoA metabolism. Measurement of CoA metabolic pools in bacteria is relatively rare. Here, acetyl CoA and butyryl CoA were present at highest concentration and the butyrate pathway intermediates at much lower concentrations, as found also in Clostridium acetobutylicum. All acyl CoAs except acetoacetyl CoA were diminished by >96% when LA was added to the medium. In contrast, the ATP pool was affected later than acyl CoA pools, and remained at about one-third of the control values, presumably due to the contribution of glycolysis.
The toxicity of PUFA in different species of ruminal bacteria was found to be related partly to whether the bacteria produced butyrate; cellulolytic bacteria were the other most sensitive species . Within the Butyrivibrio phylogenetic group, the most sensitive species were those that formed butyrate via the butyrate kinase mechanism rather than acyl CoA transferase . Thus, there seems to be a connection between PUFA toxicity and butyrate formation. A metabonomic analysis  might help to identify precisely where the PUFA act. It may also be instructive to determine why trans-11, cis-15-18:2, a product of LNA metabolism, appeared to permit growth while the other dienoic acid investigated here did not.
The influence of sodium lactate in lengthening the lag phase indicates that lactate potentiates the toxic effects of PUFA in B. fibrisolvens, as shown previously with B. proteoclasticus. Such a high concentration of lactate (70 mM) would only occur in animals suffering acidosis . The toxicity may be an osmotic effect, or due to a leakage of ions across the membrane, or may even be a metabolic effect. Lactate is a major product of glucose metabolism in B. fibrisolvens JW11 and many other butyrivibrios , and high concentrations may therefore impose metabolic feedback, further stressing bacteria affected by PUFA.
This paper explains the basis of the beneficial effect on meat and milk fatty acid composition of adding oils to the ruminant diet. Ruminal biohydrogenation is modified via differential toxicity to ruminal bacteria of different PUFA, including the fish oil fatty acids, EPA and DHA. If we can understand how selective fatty acid toxicity, or indeed other factors, affects the physiology of biohydrogenating bacteria in the rumen, we may be able to suggest new, rational dietary modifications that will eventually lead to ruminant products that are healthier for human consumption.
Bacteria and growth conditions
Butyrivibrio fibrisolvens JW11 was originally isolated from sheep as a proteolytic species , and is held in the culture collection maintained at the Rowett Institute. All transfers and incubations were carried out under O2-free CO2 and at 39°C in Hungate-type tubes . Inoculum volumes were 5% (v/v) of a fresh culture. The media used in these experiments were the liquid form of M2 medium . Fatty acids were prepared as a separate solution, sonicated for 4 min in water and added to the medium before autoclaving. Growth of bacteria was measured from the increase in optical density (OD) at 650 nm of the control tubes, in triplicate, using a Novaspec II spectrophotometer (Amersham Biosciences, UK).
The influence of fatty acids and their methyl esters was determined in two kinds of experiment. In experiments where fatty acid concentrations were measured at the end-point of the growth curve, usually in stationary phase, the tubes were freeze-dried in order to enable fatty acid extraction from the whole culture. The experiment was conducted by inoculating multiple 10-ml tubes. At each sampling time, three tubes were removed, the turbidity was determined, and the tubes were placed in a heating block at 100°C for 5 min, left to cool and frozen. One ml was taken for protein analysis and for fatty acid extraction and derivatization.
Fatty acid extraction and analysis
Extraction, derivatization of fatty acids and GC analysis of methyl esters were carried out using procedures described by Wąsowska et al. . The products from incubations with LNA were identified by comparing elution profiles and mass spectra with those identified previously from analysis of methyl and 4,4-dimethyloxazoline (DMOX) esters .
Measurement of cell integrity using propidium iodide
One ml of overnight culture was inoculated into 10 ml of M2 medium and incubated at 39°C until it reached mid-exponential phase (OD650 = 0.4, approx. 4 h). The bacterial cultures were centrifuged (3000 g, 10 min, 4°C) and the pellet was washed twice with anaerobic potassium phosphate buffer (100 mM; pH 7.0) containing 1 mM dithiothreitol (DTT). Anaerobic conditions were maintained by carrying out transfers in an anaerobic chamber with a gas phase of 80% N2, 10% CO2 and 10% H2 and temperature of 39°C. Cells were resuspended in 15 ml of the same buffer, and fatty acids and their respective methyl esters (Sigma, St. Louis, MO, USA) were added to the cell suspension to a final concentration of 50 μg ml-1. Stock solutions (1 mg ml-1) of fatty acids and methyl esters were prepared immediately before use by sonication for 4 min in anaerobic potassium phosphate buffer (100 mM, pH 7.0, containing 1 mM DTT). Untreated and heat-treated cells (100°C for 20 min) served as control samples.
Following 30 min incubation of cell suspensions with fatty acids, cell integrity was measured using PI. Ten μl of each sample were added to 985 μl of anaerobic potassium phosphate buffer, to which was added 5 μl of 1.5 mM PI (prepared in distilled water and stored at 4°C in the dark). The mixtures were incubated for 15 min at 39°C in the anaerobic chamber, then transferred to an ice-water slurry and kept in the dark for up to 45 min before being analysed for fluorescence using a fluorimeter or by flow cytometry. Fluorimetry measurements were made using a spectrofluorimeter set at λEX = 488 nm and λEM = 650 nm. Flow cytometry was carried out with a FACSCalibur flow cytometer (Becton Dickinson Immunocytometry Systems, San Jose, California, USA) equipped with an air-cooled argon ion laser emitting 15 mW of blue light at 488 nm. The red fluorescence of the PI signal was collected in the FL3 channel (>600 nm long-pass filter). FACSFlow solution (Becton Dickinson) was used as sheath fluid. The analyses were done using the low rate settings (12 μl/min).
ATP and acyl CoA pools
The influence of LA on metabolic pools in B. fibrisolvens was measured in cells growing in Roché et al.  medium in the anaerobic chamber, as follows. Fresh overnight culture (60 ml) of B. fibrisolvens JW11 was mixed with 60 ml of uninoculated medium, or uninoculated medium containing 200 μg LA ml-1, then samples (3.0 ml) were taken periodically into 1 ml of 30% (w/v) perchloric acid. After 10 min, 4 ml of KOH were added to the acidic solution, forming a precipitate of potassium perchlorate, which was removed by centrifugation (15,000 g, 15 min, 4°C). The supernatant was stored at -80°C, then subsequently thawed and ATP was measured using a luciferase preparation according to the manufacturer's (Sigma) instructions.
Acyl CoA measurements were made in parallel 120-ml control or LA-containing cultures after 20 min incubation. Cultures were maintained under CO2 and centrifuged immediately at 15,000 g for 15 min at 39°C. The pellet was stored in liquid nitrogen. Derivatization, separation, and fluorescence detection of acyl CoAs were carried out as described by Larson and Graham . Identification of acyl CoAs was carried out using mass spectrometric analysis of peaks obtained from a Hypercarb porous graphitic carbon column .
Bacterial protein was measured by a modification of the Lowry method .
All data were derived from three separate cultures. Means were compared by a Student's t-test. Measurement of the lag phase was carried out by fitting a gradient by linear regression to log(A650) vs. time during exponential phase. The lag phase was defined as the time at which the best-fit gradient passed an OD650 of 0.1, and was compared to the time at which the control cultures passed 0.1. Propidium iodide ingression was determined by 8 fluorescence measurements for each culture.
List of abbreviations
conjugated linoleic acid
polyunsaturated fatty acids
The Rowett Research Institute receives funding from the Scottish Government Rural and Environment Research and Analysis Directorate (RERAD). LCC was in receipt of a Wellcome Travelling Fellowship. We thank David Brown and Maureen Annand for their technical help and expertise. MRGM received support from the Marie Curie Training Site, 'Anaerobe'; we thank Jamie Newbold and Estelle Devillard for their help and advice. MRGM was also supported by Fundação para a Ciência e a Tecnologia (FCT), Portugal, with a PhD grant (SFRH/BD/6976/2001).
- Banks A, Hilditch TP: The glyceride structure of beef tallows. Biochem J. 1931, 25: 1168-1182.PubMed CentralView ArticlePubMedGoogle Scholar
- Menotti A, Kromhout D, Blackburn H, Fidanza F, Buzina R, Nissinen A: Food intake patterns and 25-year mortality from coronary heart disease: cross-cultural correlations in the Seven Countries Study. The Seven Countries Study Research Group. Eur J Epidemiol. 1999, 15: 507-515. 10.1023/A:1007529206050.View ArticlePubMedGoogle Scholar
- Shorland FB, Weenink RO, Johns AT: Effect of the rumen on dietary fat. Nature, Lond. 1955, 175: 1129-1130. 10.1038/1751129a0.View ArticleGoogle Scholar
- Viviani R: Metabolism of long-chain fatty acids in the rumen. Adv Lipid Res. 1970, 8: 267-346.PubMedGoogle Scholar
- Scollan ND, Choi NJ, Kurt E, Fisher AV, Enser M, Wood JD: Manipulating the fatty acid composition of muscle and adipose tissue in beef cattle. Br J Nutr. 2001, 85: 115-124. 10.1079/BJN2000223.View ArticlePubMedGoogle Scholar
- Kritchevsky D: Antimutagenic and some other effects of conjugated linoleic acid. Br J Nutr. 2000, 83: 459-465.PubMedGoogle Scholar
- Whigham LD, Cook ME, Atkinson RL: Conjugated linoleic acid: implications for human health. Pharmacol Res. 2000, 42: 503-510. 10.1006/phrs.2000.0735.View ArticlePubMedGoogle Scholar
- Jenkins TC: Regulation of lipid metabolism in the rumen. J Nutr. 1994, 124: 1372S-1376S.PubMedGoogle Scholar
- Offer NW, Marsden M, Phipps RH: Effect of oil supplementation of a diet containing a high concentration of starch on levels of trans fatty acids and conjugated linoleic acids in bovine milk. Anim Sci. 2001, 73: 533-540.Google Scholar
- Shingfield KJ, Ahvenjarvi S, Toivonen V, Arola A, Nurmela KVV, Huhtanen P, Griinari JM: Effect of dietary fish oil on biohydrogenation of fatty acids and milk fatty acid content in cows. Anim Sci. 2003, 77: 165-179.Google Scholar
- Wąsowska I, Maia M, Niedźwiedzka KM, Czauderna M, Ramalho-Ribeiro JMC, Devillard E, Shingfield KJ, Wallace RJ: Influence of fish oil on ruminal biohydrogenation of C18 unsaturated fatty acids. Br J Nutr. 2006, 95: 1199-1211. 10.1079/BJN20061783.View ArticlePubMedGoogle Scholar
- Polan CE, McNeill JJ, Tove SB: Biohydrogenation of unsaturated fatty acids by rumen bacteria. J Bacteriol. 1964, 88: 1056-1064.PubMed CentralPubMedGoogle Scholar
- Kepler CR, Hirons KP, McNeill JJ, Tove SB: Intermediates and products of the biohydrogenation of linoleic acid by Butyrivibrio fibrisolvens . J Biol Chem. 1966, 241: 1350-1354.PubMedGoogle Scholar
- Kim YJ, Liu RH, Bond DR, Russell JB: Effect of linoleic acid concentration on conjugated linoleic acid production by Butyrivibrio fibrisolvens A38. Appl Environ Microbiol. 2000, 66: 5226-5230. 10.1128/AEM.66.12.5226-5230.2000.PubMed CentralView ArticlePubMedGoogle Scholar
- Fukuda S, Furuya H, Suzuki Y, Asanuma N, Hino T: A new strain of Butyrivibrio fibrisolvens that has high ability to isomerise linoleic acid to conjugated linoleic acid. J Gen Appl Microbiol. 2005, 51: 105-113. 10.2323/jgam.51.105.View ArticlePubMedGoogle Scholar
- Paillard D, McKain N, Chaudhary LC, Walker ND, Pizette F, Koppova I, McEwan NR, Kopecny J, Vercoe PE, Louis P, Wallace RJ: Relation between phylogenetic position, lipid metabolism and butyrate production by different Butyrivibrio -like bacteria from the rumen. Ant van Leeuw. 2006, 91: 417-422. 10.1007/s10482-006-9121-7.View ArticleGoogle Scholar
- Maia MRG, Chaudhary LC, Figueres L, Wallace RJ: Metabolism of polyunsaturated fatty acids and their toxicity to the microflora of the rumen. Ant van Leeuw. 2006, 91: 303-314. 10.1007/s10482-006-9118-2.View ArticleGoogle Scholar
- Moon CD, Pacheco DM, Kelly WJ, Leahy SC, Li D, Kopecny J, Attwood GT: Reclassification of Clostridium proteoclasticum as Butyrivibrio proteoclasticus comb. nov., a butyrate-producing ruminal bacterium. Int J System Evol Microbiol. 2008, 58: 2041-2045. 10.1099/ijs.0.65845-0.View ArticleGoogle Scholar
- Stewart CS, Flint HJ, Bryant MP: The rumen bacteria. The rumen microbial ecosystem. Edited by: Hobson PN, Stewart CS. 1997, London: Chapman and Hall, 10-72.View ArticleGoogle Scholar
- Hazlewood GP, Orpin CG, Greenwood Y, Black ME: Isolation of proteolytic rumen bacteria by use of selective medium containing leaf fraction 1 protein (ribulose bis phosphate carboxylase). Appl Environ Microbiol. 1983, 45: 1780-1784.PubMed CentralPubMedGoogle Scholar
- Wallace RJ, Brammall ML: The role of different species of rumen bacteria in the hydrolysis of protein in the rumen. J Gen Microbiol. 1985, 131: 821-832.Google Scholar
- Harfoot CG, Hazlewood GP: Lipid metabolism in the rumen. The rumen microbial ecosystem. Edited by: Hobson PN, Stewart CS. 1997, London: Chapman and Hall, 382-426.View ArticleGoogle Scholar
- Wallace RJ, Chaudhary LC, McKain N, McEwan NR, Richardson AJ, Vercoe PE, Walker ND, Paillard D: Clostridium proteoclasticum: a ruminal bacterium that forms stearic acid from linoleic acid. FEMS Microbiol Lett. 2006, 265: 195-201. 10.1111/j.1574-6968.2006.00487.x.View ArticleGoogle Scholar
- White RW, Kemp P, Dawson RMC: Isolation of a rumen bacterium that hydrogenates oleic acid as well as linoleic and linolenic acid. Biochem J. 1970, 116: 767-768.PubMed CentralView ArticlePubMedGoogle Scholar
- Kemp P, White RW, Lander DJ: The hydrogenation of unsaturated fatty acids by five bacterial isolates from the sheep rumen, including a new species. J Gen Microbiol. 1975, 90: 100-114.View ArticlePubMedGoogle Scholar
- Hazlewood GP, Kemp P, Lauder D, Dawson RMC: C18 unsaturated fatty acid hydrogenation patterns of some rumen bacteria and their ability to hydrolyse exogenous phospholipid. Br J Nutr. 1976, 35: 293-297. 10.1079/BJN19760034.View ArticlePubMedGoogle Scholar
- Henderson C: The effects of fatty acids on pure cultures of rumen bacteria. J Agric Sci Camb. 1973, 81: 107-112. 10.1017/S0021859600058378.View ArticleGoogle Scholar
- Marounek M, Skrivanova V, Savka O: Effect of caprylic, capric and oleic acid on growth of rumen and rat caecal bacteria. J Anim Feed Sci. 2002, 11: 507-516.Google Scholar
- Galbraith H, Miller TB, Paton AM, Thompson JK: Antibacterial activity of long-chain fatty acids and the reversal with calcium, magnesium, ergocalciferol and cholesterol. J Appl Bacteriol. 1971, 34: 803-813.View ArticlePubMedGoogle Scholar
- Kemp P, Lander DJ: Hydrogenation in vitro of α-linolenic acid to stearic acid by mixed cultures of pure strains of rumen bacteria. J Gen Microbiol. 1984, 130: 527-533.Google Scholar
- Kemp P, Lander DJ, Gunstone FD: The hydrogenation of some cis- and trans-octadecenoic acids to stearic acid by a rumen Fusocillus sp. Br J Nutr. 1984, 52: 165-170. 10.1079/BJN19840083.View ArticlePubMedGoogle Scholar
- Lennarz WJ: Lipid metabolism in the bacteria. Adv Lipid Res. 1966, 4: 175-225.PubMedGoogle Scholar
- Hughes PE, Hunter WJ, Tove SB: Biohydrogenation of unsaturated fatty acids. Purification and properties of cis-9, trans-11-octadecadienoate reductase. J Biol Chem. 1982, 257: 3643-3649.PubMedGoogle Scholar
- Keweloh H, Heipieper HJ: Trans unsaturated fatty acids in bacteria. Lipids. 1996, 31: 129-137. 10.1007/BF02522611.View ArticlePubMedGoogle Scholar
- Cheng K-J, Costerton JW: Ultrastructure of Butyrivibrio fibrisolvens - a Gram-positive bacterium?. J Bacteriol. 1977, 129: 1506-1512.PubMed CentralPubMedGoogle Scholar
- Mitchell P: Keilin's respiratory chain concept and its chemiosmotic consequences. Science. 1979, 206: 1148-1159. 10.1126/science.388618.View ArticlePubMedGoogle Scholar
- Nichols DG: Bioenergetics: an introduction to the chemiosmotic theory. 1982, Academic Press, London, 190-Google Scholar
- Rottenberg H, Hashimoto K: Fatty acid uncoupling of oxidative phosphorylation in rat liver mitochondria. Biochemistry. 1986, 25: 1747-1755. 10.1021/bi00355a045.View ArticlePubMedGoogle Scholar
- Rottenberg H, Steiner-Mordoch S: Fatty acids decouple oxidative phosphorylation by dissipating intramembranal protons without inhibiting ATP synthesis driven by the proton electrochemical gradient. FEBS Lett. 1986, 202: 314-318. 10.1016/0014-5793(86)80708-6.View ArticlePubMedGoogle Scholar
- Boynton ZL, Bennett GN, Rudolph FB: Intracellular concentrations of Coenzyme A and its derivatives from Clostridium acetobutylicum ATCC 824 and their roles in enzyme regulation. Appl Environ Microbiol. 1994, 60: 39-44.PubMed CentralPubMedGoogle Scholar
- Nicholson JK, Lindon JC, Holmes E: 'Metabonomics': understanding the metabolic responses of living systems to pathophysiological stimuli via multivariate statistical analysis of biological NMR spectroscopic data. Xenobiotica. 1999, 29: 1181-1189. 10.1080/004982599238047.View ArticlePubMedGoogle Scholar
- Owens FN, Secrist DS, Hill WJ, Gill DR: Acidosis in cattle: A review. J Anim Sci. 1998, 76: 275-286.PubMedGoogle Scholar
- Hungate RE: A roll tube method for cultivation of strict anaerobes. Methods in Microbiology. Edited by: Norris JR, Ribbons DW. 1969, London: Academic Press, 3B: 117-132. full_text.Google Scholar
- Hobson PN: Rumen bacteria. Methods in Microbiology. Edited by: Norris JR, Ribbons DW. 1969, London: Academic Press, 3B: 133-139. full_text.Google Scholar
- Roché C, Albertyn H, Van Gylswyk , Kistner A: The growth response of cellulolytic acetate-utilising and acetate-producing butyrivibrio's to volatile fatty acids and other nutrients. J Gen Microbiol. 1973, 78: 253-260.View ArticlePubMedGoogle Scholar
- Larson TR, Graham IA: Technical Advance: a novel technique for the sensitive quantification of acyl CoA esters from plant tissues. Plant. 2001, 25: 115-125. 10.1046/j.1365-313x.2001.00929.x.View ArticleGoogle Scholar
- Ishizaki K, Larson TR, Schauer N, Fernie AR, Graham IA, Leaver CJ: The critical role of Arabidopsis electron-transfer flavoprotein:ubiquinone oxidoreductase during dark-induced starvation. Plant Cell. 2005, 17: 2587-2600. 10.1105/tpc.105.035162.PubMed CentralView ArticlePubMedGoogle Scholar
- Herbert D, Phipps PJ, Strange RE: Chemical analysis of microbial cells. Methods in Microbiology. Edited by: Norris JR, Ribbons DW. 1971, London: Academic Press, 5B: 209-344. full_text.Google Scholar