Steering Endogenous Butyrate Production in the Intestinal Tract of Broilers as a Tool to Improve Gut Health
- Department of Pathology, Bacteriology and Avian Diseases, Ghent University, Merelbeke, Belgium
The ban on antimicrobial growth promoters and efforts to reduce therapeutic antibiotic usage has led to major problems of gastrointestinal dysbiosis in livestock production in Europe. Control of dysbiosis without the use of antibiotics requires a thorough understanding of the interaction between the microbiota and the host mucosa. The gut microbiota of the healthy chicken is highly diverse, producing various metabolic end products, including gases and fermentation acids. The distal gut knows an abundance of bacteria from within the Firmicutes Clostridium clusters IV and XIVa that produce butyric acid, which is one of the metabolites that are sensed by the host as a signal. The host responds by strengthening the epithelial barrier, reducing inflammation, and increasing the production of mucins and antimicrobial peptides. Stimulating the colonization and growth of butyrate-producing bacteria thus may help optimizing gut health. Various strategies are available to stimulate butyrate production in the distal gut. These include delivery of prebiotic substrates that are broken down by bacteria into smaller molecules which are then used by butyrate producers, a concept called cross-feeding. Xylo-oligosaccharides (XOS) are such compounds as they can be converted to lactate, which is further metabolized to butyrate. Probiotic lactic acid producers can be supplied to support the cross-feeding reactions. Direct feeding of butyrate-producing Clostridium cluster IV and XIVa strains are a future tool provided that large scale production of strictly anaerobic bacteria can be optimized. Current results of strategies that promote butyrate production in the gut are promising. Nevertheless, our current understanding of the intestinal ecosystem is still insufficient, and further research efforts are needed to fully exploit the capacity of these strategies.
For many years, broiler intestinal health was supported by the widespread use of antimicrobial growth promoters (AGPs). These AGPs are antibiotic substances that were added to the feed at subtherapeutic levels, leading to improved animal performance. In the European Union, the use of AGPs was banned in 2006 while the Center for Veterinary Medicine of the US Food and Drug Administration, in 2012, wrote a “Guidance for Industry” document recommending that antibiotics should only be used in case of specific diseases and not for growth promotion. The most important reason for these precautionary measures was the likelihood that AGPs may increase antimicrobial resistance in bacteria, in some cases followed by introduction of these bacteria in humans (1). Most likely intestinal health problems in the chicken have been masked partly by the routine use of AGPs. Since the ban of AGPs in Europe alternative strategies for control of intestinal health have become a focus of research. These research efforts have revealed the complexity of the intestinal ecosystem. The gut indeed is an organ that contains many different cell types and exerts many different functions (2). In addition, the composition of the gut microbiota is diverse and varies depending on different factors, including the feed composition. The interaction between the host and the beneficial microbes in the intestine is mutualistic, as the host provides an anaerobic shelter and nutrients for the bacteria, which in turn provide enzymes that help digesting polysaccharides and other complex molecules (3). Nonetheless, the intestinal tract also contains facultative pathogenic microorganisms, which may be harmful and even life-threatening to the host under certain conditions. The challenge for the intestinal immune system is thus to simultaneously create a firm barrier and a powerful defense against the pathogenic bacteria, while at the same time, foster the beneficial bacteria and create an open entrance for the nutrients. These apparently conflicting tasks are taken up by the intestinal mucosa forming the so-called intestinal barrier that receives signals from the intestinal bacteria (4). Microbial signals can originate from cell wall components, like lipopolysaccharides (LPS) and flagellin, DNA fragments, and metabolites such as short-chain fatty acids (SCFAs). Those signals can have proinflammatory or anti-inflammatory effects, depending on the signal (5). One important signal derived from the beneficial microbes is butyrate.
When considering signals derived from bacterial fermentation, butyric acid has been shown to be the main driving force toward an optimal gut health. The molecule exerts beneficial effects in the physiological concentration range (6, 7). Numerous butyrate products are available on the market in a wide range of formulations. However, another possibility to increase butyric acid in the gut is by stimulating the endogenous production of butyrate by the gut microbiota. This review focuses on the methods on how to increase the endogenous production of butyrate in the intestinal tract of broilers in order to improve gut health.
Role of the Intestinal Barrier in Gut Health
The luminal side of the intestinal wall is lined with absorptive epithelial cells, needed for water and nutrient uptake, which form a semipermeable barrier between the outside world (the gut lumen) and the internal host tissues. This semipermeable barrier is not only formed by the cell membranes of the epithelial cells but also by tight junctions that connect neighboring epithelial cells (8). These connections are regulated at different levels (e.g., by cytokines). The permeability of the intestinal epithelial cell layer can be affected by epithelial cell death and also by luminal signals that increase the epithelial layer permeability by affecting the tight junctions and thus cause loss of integrity of this important barrier (4). This loss of integrity can have detrimental effects. First, it causes an efflux of host proteins (“leaky gut”) into the lumen and can cause luminal molecules, including toxins, and microorganisms, to reach the basal side of the epithelial layer. Through coevolution, the host has developed the capacity to become tolerant to most bacteria present in the lumen at the apical side of the epithelial cells. However, bacterial components that closely interact with epithelial cells from the basolateral side do trigger an inflammatory response. This is mediated by the binding of pathogen-associated molecular patterns, such as LPS and flagellin, to the so-called Toll-like receptors that trigger the cascade of proinflammatory signals (9). It is evident that the loss of intestinal epithelial integrity and its consequences will have an effect on animal performance.
In addition to the absorptive epithelial cells, other cell types are present in the lining of the gut wall. These include mucin-producing goblet cells and antimicrobial peptide (AMP)-producing paneth cells in the crypts (10). Both cell types are very important in innate defenses. Enteroendocrine cells can also be found in the epithelial lining, secreting peptide hormones into the bloodstream. These peptide hormones have a variety of functions, including effects on epithelial cell proliferation, inflammation, and consequently intestinal barrier integrity. One of these hormones is glucagon-like peptide-2 (GLP-2), a hormone that is important in maintaining epithelial integrity (11). The enteroendocrine cells are activated by various luminal signals, including bacterial signals (see below).
Underneath the epithelial lining, many other cell types are present which together form the lamina propria of the intestinal mucosa. These cells include, among others, fibroblasts and endothelial cells. Immune cells are also present in the mucosa, both in organized lymphoid tissues and scattered between the other cells. All non-epithelial cell types are responsive to luminal triggers, whether transmitted by epithelial cell signals, including enteroendocrine cell hormones, or not, and thus can influence other cell types by themselves. Thus, intestinal barrier integrity, inflammation, and gut function are influenced by luminal signals, many of which are produced by the microbiota (12). The composition of the microbiota and the metabolites the bacteria produce are hence crucial for gut health.
Effects of Butyrate
One of the major terminal metabolites of intestinal bacteria is butyrate. The effects of butyrate on intestinal health have already been described in detail in many reports (6, 13). The main targets of butyrate are briefly described in the following paragraph. Supplementation of butyrate in the feed can beneficially influence growth performance and intestinal villus structure in broiler chickens (14). Presence of butyrate in the intestine plays a role in the control of pathogens such as Salmonella Enteritidis and Clostridium perfringens. Reduction of Salmonella enterica serovar Enteritidis colonization and shedding in chickens has been reported (15, 16), as well as a decrease of necrotic lesions induced by C. perfringens in the small intestine (17). In addition to the role of butyrate in growth performance and pathogen control, butyrate also has anti-inflammatory properties. One of the mechanisms is inhibition of nuclear factor-kappa B activation, resulting in decreased expression of proinflammatory cytokines (18, 19). As described above, the intestinal barrier plays an important role in maintaining intestinal health. Butyrate has an effect on several components of this barrier (13, 20), such as the tight junctions (21). Butyrate upregulates AMP-activated protein kinase, which regulates the assembly of tight junctions (22). The mucin-producing goblet cells in the small intestine and distal gastrointestinal tract are also influenced by the presence of butyrate (23, 24). Butyrate-induced expression of MUC2 genes results in secretion of mucin, a glycoprotein, which forms a protective layer on the enterocytes (23, 25). AMP-producing paneth cells in the crypts are another cell type influenced by butyrate. Expression of AMPs, such as cathelicidins and defensins, is upregulated upon supplementation of butyric acid (26, 27). Finally, it is assumed that butyrate affects enteroendocrine L-cells secreting GLP-2 (28). Beneficial effects of GLP-2 on general gut health, such as the stimulation of intestinal crypt cell proliferation and the reduction of apoptosis in the crypt compartment, have been described for several animal species (29, 30). Information about the function of GLP-2 in chickens is scarce. Honda et al. (31) reported suppressed feed intake after intracerebroventricular administration of GLP-2 in chickens, which suggests that GLP-2 plays a role in regulating appetite (31). Daily intraperitoneal injection of GLP-2 in healthy broiler chickens improves absorptive function of the small intestine and has a positive effect on growth performance (32). GLP-2 receptors are thought to be present in chicken proventriculus, duodenum, jejunum, ileum, cecum, and colon, as detected by PCR (33). L-cells containing GLP-2 are mainly found in the crypts of the distal ileum and the proximal jejunum (34). This information could prove useful in unraveling the functions of GLP-2 in birds and in finding out which physiological triggers lead to secretion of the hormone (35). In humans, it is reported that butyrate enhances GLP-2 secretion and increases GLP-2 plasma concentration (35, 36). However, studies in chickens are lacking, and further research is necessary to yield conclusive information about the effect of butyrate on the release of GLP-2 in chickens.
The Intestinal Microbiota with Focus on Endogenous Butyrate Production
The composition of the microbiota in the gut of chickens depends on the age and the gastrointestinal segment, i.e., there is both a temporal as well as a spatial variation (37). In general, the diversity of the microbiota increases with age. The composition of microbiota differs between the different segments of the chicken gut. In general, low numbers of bacteria are found in the proximal parts of the gut (stomach, duodenum, jejunum, <103 cfu/g content), while the numbers increase toward the distal ileum and ceca, the latter harboring more than 1010 bacteria/g of content. In addition, the diversity increases significantly toward the distal gut. While only a limited diversity can be observed in the small intestine, with lactobacilli often dominant, the ceca harbor a large number of different bacterial groups (38). The cecal ecosystem of healthy subjects is dominated by bacteria belonging to the phyla Bacteroidetes and Firmicutes, together comprising more than 80% of the microbiota. The former contains many polysaccharide-degrading bacterial species, while the latter contains a variety of bacterial families, of which the Ruminococcaceae (Clostridium cluster IV) and Lachnospiraceae (Clostridium cluster XIVa) families are capable of fermenting various substrates to butyrate. The bacterial community has the genetic potential to carry out an enormous number of physiological functions (37). They can play an important role in both immune and digestive functions. Commensal bacteria can exert anti-inflammatory properties by producing SCFA (see below). Moreover, the mucosal architecture, mucus composition, and production can be affected by the presence of the gastrointestinal bacteria (39). The number of microbial genes in the gut of a chicken exceeds the number of chicken genes. Together these form a so-called “hologenome” (40).
Butyrate-Producing Bacteria and Bacteria That Promote/Inhibit Butyrate Production
While a large variety of bacteria can produce acetic acid, the most important butyric acid-producing bacteria belong to a limited number of families, including the Ruminococcaceae and Lachnospiraceae (41). These families contain strictly anaerobic bacteria that are highly abundant in the gut of healthy chickens, as well as mammals. Other Clostridium clusters, including clusters I and XVI, contain butyrate producers, but the level of butyrate produced is much lower in comparison with strains from cluster IV and XIVa (42, 43). Individual butyrate-producing strains isolated from chicken ceca have been characterized (44, 45). In 2011, a first study specifically investigated the diversity of butyrate-producing bacteria from chicken ceca. 16S rRNA gene sequence analysis of isolates revealed members of Clostridium clusters IV, XIVa, XIVb, and XVI (42). When butyrate-producing bacteria are present in a sufficiently high concentration, the epithelial barrier integrity will be stronger, the epithelial cells will proliferate more and thus the villi will be longer. Moreover, inflammatory reactions will be reduced, while the stimulation of regulatory T-lymphocytes will yield a state of tolerance toward non-harmful bacteria (46). Butyrate is mainly synthesized via the reductive acetyl-coenzyme A pathway (47). Via a four-step pathway, acetyl-CoA is converted to the intermediate butyryl-CoA and further to butyrate. The final step or actual butyrate formation in its synthesis is mostly catalyzed by butyryl-CoA:acetate CoA-transferase and is used by several families of the healthy gut microbiota, dominated by Lachnospiraceae and Ruminococcaceae (48, 49). Another, but less frequently used, enzyme in the final step is butyrate kinase that produces butyrate from butyrylphosphate that is derived after phosphorylation of butyryl-CoA (7). Recently, it has been hypothesized that a propionate CoA transferase related to the enzyme of Clostridium propionicum is responsible for butyrate formation in members of the family Erysipelotrichaceae (42). In addition, three other butyrate-producing pathways using amino acids as major substrates are known. These pathways, only present in 20% of potential butyrate producers, are the lysine, 4-aminobutyrate, and glutarate pathways (47).
Other Microorganisms That May Interact with Butyrate Production
The variety of metabolic functions of the intestinal microbiome encompasses degradation of complex substrates (polysaccharides, proteins, and fat), fermentation of substrates to yield acidic compounds, immunomodulation, communication with other bacteria, and much more. To break down complex substrates, the bacteria form a food web, with different species and strains involved in different steps of the substrate utilization process (50). In a simplified model, complex substrates such as polysaccharides, including arabinoxylans, pectins, and cellulose, are converted to oligosaccharides by specific bacterial populations such as lactobacilli and some Bacteroides species, among others. These oligosaccharides [e.g., arabinoxylan-oligosaccharides (AXOS)] are then used by other bacterial groups to produce lactic acid, hydrogen, and SCFAs such as acetic, propionic, and butyric acid (41). The system in which bacteria convert substrates to products that are converted by other bacteria is called cross-feeding. This is an important mechanism, clearly showing the need of a diverse bacterial community, in order to be able to degrade substrates (51, 52). In case of dysbiosis, an unfavorable shift in the composition of the microbiota occurs, leading to deficiencies in certain crucial steps in certain pathways, yielding changes in the bacterial metabolites produced in the gut (53). Bacteria that promote butyrate production through the production of intermediate metabolites, as well as bacteria that inhibit butyrate production by competition for substrates can be present in the gut. For example, the underlying mechanism by which lactic acid bacteria (LABs) can be beneficial can be explained by the effects of butyrate, considering that the lactic acid produced by these bacteria is then further consumed by Clostridium cluster XIV strains to produce butyrate (48). Lactic acid is toxic by itself when present in high concentrations and only has a benefit when it is converted (54). Sulfate-reducing bacteria (SRBs) compete for lactate with butyrate-producing bacteria from Clostridium cluster XIVa, with the outcome of this competition being a crucial factor for gut health. Apart from this, SRBs also have to compete for hydrogen with hydrogenotrophic acetogenic and methanogenic bacteria (55). They produce hydrogen sulfide as a terminal metabolite. Hydrogen sulfide, with proven cell death-inducing effects on intestinal epithelial cells, is a clearly toxic metabolite (56). One can thus conclude that a complex interaction between different bacterial populations for specific substrates exists, and the outcome of this interaction can drive the microbiota either to produce beneficial metabolites which promote gut health, or toward production of toxic metabolites.
Tools to Stimulate Endogenous Butyrate Production
The term probiotics was first defined by FOA/WHO in 2001, and at the end of 2013, the definition was worded more grammatically correct as “live microorganisms that, when administered in adequate amounts, confer a health benefit on the host” (57). The majority of bacterial probiotics consist of LABs, mainly from the Lactobacillus, Bifidobacterium, Enterococcus, and Streptococcus genera (58, 59). As discussed above, lactic acid can be consumed by butyrate-producing bacteria to produce butyrate (48). Different types of products are currently available on the market. Beside single-strains, multi-strain products are available, as well as competitive exclusion (CE) products, which contain a freeze-dried mixture of gut content. The main purpose of CE products is replacing the natural route of microbiota succession, while probiotics enhance the functions of existing microbiota. Besides, only defined CE products can be registered for which the identities of the bacteria in the mixture are known to be safe for chickens and humans (60).
Reports of the effect of probiotics on animal performance have been published (61, 62), and studies on the beneficial effect on pathogen colonization and disease reduction are widely available (63–65). However, positive effects are not observed in all studies. One of the reasons for the inconsistency of observed beneficial effects may be that success depends partly on the conditions of the study, i.e., feed formulae and feed ingredients, management factors, and presence or absence of stress factors and challenge conditions. Indeed, unpublished data from our laboratory show that the efficacy of probiotics is highly dependent on the model used. However, based on the above described data, attempts could be made to develop probiotics that stimulate butyrate production in the intestinal tract, either directly or through cross-feeding.
Butyrate-Producing Bacteria as Probiotic Strains
Most butyrate-producing bacteria belong to the Clostridium clusters IV and XIVa (66, 67) and play an important role in maintaining a healthy gut primarily through production of butyrate (7). These bacteria are less abundant in the gut of people suffering from inflammatory bowel disease (IBD) as compared to healthy persons (68). More specifically, Butyricicoccus pullicaecorum and Faecalibacterium prausnitzii, species belonging to Clostridium cluster IV, have been shown to be less abundant in the gut of IBD patients (68, 69). Thus, oral administration of these strains as probiotics might counteract IBD inflammation. At the moment, no specific studies are available in literature that show beneficial effects of butyrate-producing bacteria from Clostridium clusters IV and XIVa as probiotic candidates in poultry. However, Clostridium butyricum from Clostridium cluster I, administered as a component of a tri-strain probiotic, significantly improved body weight gain and reduced feed conversion rate in broiler chickens (70). Similar results have been reported with supplementation of C. butyricum in the feed as single strain probiotic (71).
A major problem with the production of butyrate-producing bacteria as probiotic is the cultivation, as these microorganisms require strict anaerobic conditions (72). Another issue is that most poultry feed is pelleted, and probiotic strains are exposed to high temperatures during this process. Thus, ideally the probiotic strains should be heat-stable, for example, through spore formation (73). Unfortunately, most butyrate-producing bacteria seem to lack this characteristic.
Other Microorganisms as Probiotic Strains Increasing Butyrate Concentration
Instead of direct administration of butyrate-producing bacteria to the bird, attempts could be made to use strains that stimulate butyrate production by Clostridium cluster IV and XIVa strains. The Clostridium cluster XIVa strains consume lactic acid to produce butyric acid. Therefore, LABs could be useful probiotics for their property of indirect stimulation of butyrate production. This cross-feeding mechanism may explain the beneficial effects of lactobacilli and bifidobacteria (70, 74). Addition of lactobacilli in an in vitro fermentation system of cecal broiler content increases butyrate concentration (75). This suggests that lactobacilli, as probiotic bacteria, stimulate butyrate-producing bacteria in the chicken cecum. These effects are, however, hitherto not investigated in vivo in chickens.
The definition of prebiotics as proposed by Gibson et al. (76) is “Selectively fermented ingredients that allow specific changes, both in the composition and/or activity of the gastrointestinal microflora that confer benefits upon host wellbeing and health” (76). Several prebiotics induce beneficial effects on broiler performance and pathogen control (77, 78). Most published studies involve oligosaccharides, such as fructo-oligosaccharides (FOS), galacto-oligosaccharides (GOS), arabinoxylo-oligosaccharides (AXOS), xylo-oligosaccharides (XOS), and raffinose family oligosaccharides (RFOs) (79). Prebiotics are complex molecules because of the chain length, the nature of the sugar bonds, and the nature of the side chains on the saccharides. These characteristics can affect their function as prebiotic (80). Prebiotics need to be converted into metabolites by the microbiota in the gut. Because they are saccharides, their end products will be SCFAs, lactate, and gases, and thus the beneficial effect can theoretically be evaluated or predicted by analyzing these metabolites.
Prebiotics Used By Butyrate-Producing Bacteria and Other Microorganisms
Prebiotics that stimulate colonization and activity of butyrate-producing Clostridium cluster IV and XIVa populations are considered to be beneficial. For example, our group showed that XOS supplementation to a broiler diet increases the number of lactobacilli and Clostridium cluster XIVa strains in the distal gut, thereby stimulating the cross-feeding between both groups, so that lactate is converted into butyrate (78). Different studies report improved growth performance and an increase of Lactobacillus and Bifidobacterium bacteria in the gut of broilers after administration of oligosaccharides (81–83). After supplementation of AXOS in the diet, a decrease of Salmonella Enteritidis and improved feed conversion rate is reported in poultry (44, 84). Contradictory results have been published with FOS supplementation in broilers. Several studies report a decrease of pathogen colonization, i.e., Salmonella, C. perfringens, and Escherichia coli, in the cecum of broilers (81, 85, 86), and an increase of Bifidobacterium spp. and Lactobacillus spp. (81). Other studies in broilers report no effect at all (87, 88). These discrepancies could be explained by differences in age, diet composition, and concentration of FOS in the diet. As discussed above, it can be hypothesized that the observed beneficial effects are at least partly due to the bacteria supporting the cross-feeding leading toward production of butyrate.
A large number of experimental and field trials in broilers have already been carried out, using a variety of feed additives. The most commonly measured outcome parameter is performance. Some studies were also done to determine the effect on pathogen colonization. The approach was mostly empirical and the products were therefore mainly developed without a clear understanding of the mode of action underlying the hoped-for beneficial effects. The only way to develop products with an enhanced activity as compared to the already existing products will be based on a thorough understanding of the intestinal ecosystem. Identification of the microbiota components that are crucial to gut health is ongoing and forms an essential part of the proper development of additives that support gut health (67). This needs to be done in both ways, i.e., identifying both the beneficial microbes as well as the harmful ones. Current knowledge indicates that butyrate-producing bacteria and their metabolite butyrate improve gut health in the physiological range (6). The amount of butyrate produced by the microbes in the lower intestinal tracts is impressive, considering that more than 50% of the microbiome is composed of butyrate producers (7). Deficiencies in butyrate production by the microbiota for whatever reason always seem to lead to inflammation in the intestinal tract (13). Providing a butyrate supplement in the feed only gives a partial answer to the problem, as the amount that can be added to the feed is limited. Thus, there is ample reason to try and stimulate endogenous butyrate production. This can be achieved by using feed additives, i.e., prebiotics that support the proliferation and the metabolic activities of the butyrate producers. Another possible strategy to stimulate endogenous butyrate production is by direct feeding of butyrate-producing bacteria. However, most probably a range of other metabolites exists with unknown mechanisms and influences on gut health. There is a need to investigate the specific effects of the different bacteria and metabolites that are found to play a role in gut health. Bacterial culturing is a crucial tool to foster our understanding of the intestinal ecosystem and essential in studying the effect of a specific species or strain on gut health parameters (2). Only a small minority of the microbial species residing in the gut has ever been cultured, and therefore isolation and characterization of new bacterial species from the gut will yield useful information (89).
Finally, the feed–microbiota–host interactions are extremely complex, but expertise on how to steer this interaction is growing rapidly. One way is to increase the abundance of butyrate-producing bacteria from Clostridium cluster IV and XIVa. In the future, many more health promoting as well as harmful bacterial groups and metabolites will doubtlessly be discovered. This will further contribute to optimizing gut health and animal performance.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
1. Butaye P, Devriese LA, Haesebrouck F. Antimicrobial growth promoters used in animal feed: effects of less well known antibiotics on gram-positive bacteria. Clin Microbiol Rev (2003) 16(2):175–88. doi: 10.1128/Cmr.16.2.175-188.2003
6. Guilloteau P, Martin L, Eeckhaut V, Ducatelle R, Zabielski R, Van Immerseel F. From the gut to the peripheral tissues: the multiple effects of butyrate. Nutr Res Rev (2010) 23(2):366–84. doi:10.1017/S0954422410000247
7. Louis P, Flint HJ. Diversity, metabolism and microbial ecology of butyrate-producing bacteria from the human large intestine. FEMS Microbiol Lett (2009) 294(1):1–8. doi:10.1111/j.1574-6968.2009.01514.x
13. Canani RB, Costanzo MD, Leone L, Pedata M, Meli R, Calignano A. Potential beneficial effects of butyrate in intestinal and extraintestinal diseases. World J Gastroenterol (2011) 17(12):1519–28. doi:10.3748/wjg.v17.i12
15. Van Immerseel F, Boyen F, Gantois I, Timbermont L, Bohez L, Pasmans F, et al. Supplementation of coated butyric acid in the feed reduces colonization and shedding of Salmonella in poultry. Poult Sci (2005) 84(12):1851–6. doi:10.1093/ps/84.12.1851
16. Fernandez-Rubio C, Ordonez C, Abad-Gonzalez J, Garcia-Gallego A, Honrubia MP, Mallo JJ, et al. Butyric acid-based feed additives help protect broiler chickens from Salmonella enteritidis infection. Poult Sci (2009) 88(5):943–8. doi:10.3382/ps.2008-00484
17. Timbermont L, Lanckriet A, Dewulf J, Nollet N, Schwarzer K, Haesebrouck F, et al. Control of Clostridium perfringens-induced necrotic enteritis in broilers by target-released butyric acid, fatty acids and essential oils. Avian Pathol (2010) 39(2):117–21. doi:10.1080/03079451003610586
18. Inan MS, Tolmacheva V, Wang QS, Rosenberg DW, Giardina C. Transcription factor NF-kappaB participates in regulation of epithelial cell turnover in the colon. Am J Physiol Gastrointest Liver Physiol (2000) 279(6):G1282–91.
19. Place RF, Noonan EJ, Giardina C. HDAC inhibition prevents NF-kappa B activation by suppressing proteasome activity: down-regulation of proteasome subunit expression stabilizes I kappa B alpha. Biochem Pharmacol (2005) 70(3):394–406. doi:10.1016/j.bcp.2005.04.030
20. Hamer HM, Jonkers D, Venema K, Vanhoutvin S, Troost FJ, Brummer RJ. Review article: the role of butyrate on colonic function. Aliment Pharmacol Ther (2008) 27(2):104–19. doi:10.1111/j.1365-2036.2007.03562.x
21. Mitic LL, Van Itallie CM, Anderson JM. Molecular physiology and pathophysiology of tight junctions I. Tight junction structure and function: lessons from mutant animals and proteins. Am J Physiol Gastrointest Liver Physiol (2000) 279(2):G250–4.
22. Peng L, Li ZR, Green RS, Holzman IR, Lin J. Butyrate enhances the intestinal barrier by facilitating tight junction assembly via activation of AMP-activated protein kinase in Caco-2 cell monolayers. J Nutr (2009) 139(9):1619–25. doi:10.3945/jn.109.104638
23. Smirnov A, Perez R, Amit-Romach E, Sklan D, Uni Z. Mucin dynamics and microbial populations in chicken small intestine are changed by dietary probiotic and antibiotic growth promoter supplementation. J Nutr (2005) 135(2):187–92.
24. Hatayama H, Iwashita J, Kuwajima A, Abe T. The short chain fatty acid, butyrate, stimulates MUC2 mucin production in the human colon cancer cell line, LS174T. Biochem Biophys Res Commun (2007) 356(3):599–603. doi:10.1016/j.bbrc.2007.03.025
25. Willemsen LE, Koetsier MA, van Deventer SJ, van Tol EA. Short chain fatty acids stimulate epithelial mucin 2 expression through differential effects on prostaglandin E(1) and E(2) production by intestinal myofibroblasts. Gut (2003) 52(10):1442–7. doi:10.1136/gut.52.10.1442
26. Goitsuka R, Chen CL, Benyon L, Asano Y, Kitamura D, Cooper MD. Chicken cathelicidin-B1, an antimicrobial guardian at the mucosal M cell gateway. Proc Natl Acad Sci U S A (2007) 104(38):15063–8. doi:10.1073/pnas.0707037104
27. Sunkara LT, Achanta M, Schreiber NB, Bommineni YR, Dai G, Jiang W, et al. Butyrate enhances disease resistance of chickens by inducing antimicrobial host defense peptide gene expression. PLoS One (2011) 6(11):e27225. doi:10.1371/journal.pone.0027225
30. Guan X, Karpen HE, Stephens J, Bukowski JT, Niu S, Zhang G, et al. GLP-2 receptor localizes to enteric neurons and endocrine cells expressing vasoactive peptides and mediates increased blood flow. Gastroenterology (2006) 130(1):150–64. doi:10.1053/j.gastro.2005.11.005
31. Honda K, Saneyasu T, Yamaguchi T, Shimatani T, Aoki K, Nakanishi K, et al. Intracerebroventricular administration of novel glucagon-like peptide suppresses food intake in chicks. Peptides (2014) 52:98–103. doi:10.1016/j.peptides.2013.12.008
32. Hu XF, Guo YM, Huang BY, Bun S, Zhang LB, Li JH, et al. The effect of glucagon-like peptide 2 injection on performance, small intestinal morphology, and nutrient transporter expression of stressed broiler chickens. Poult Sci (2010) 89(9):1967–74. doi:10.3382/ps.2009-00547
33. Mo C, Zhong Y, Wang Y, Yan Z, Li J. Characterization of glucagon-like peptide 2 receptor (GLP2R) gene in chickens: functional analysis, tissue distribution, and developmental expression profile of GLP2R in embryonic intestine. Domest Anim Endocrinol (2014) 48:1–6. doi:10.1016/j.domaniend.2014.01.002
34. Monir MM, Hiramatsu K, Nishimura K, Takemoto C, Watanabe T. Distribution of glucagon-like peptide (GLP)-2-immunoreactive cells in the chicken small intestine: antigen retrieval immunohistochemistry. J Vet Med Sci (2014) 76(4):565–8. doi:10.1292/jvms.13-0513
36. Mangian HF, Tappenden KA. Butyrate increases GLUT2 mRNA abundance by initiating transcription in Caco2-BBe cells. JPEN J Parenter Enteral Nutr (2009) 33(6):607–17; discussion 17. doi:10.1177/0148607109336599
37. Stanley D, Hughes RJ, Moore RJ. Microbiota of the chicken gastrointestinal tract: influence on health, productivity and disease. Appl Microbiol Biotechnol (2014) 98(10):4301–10. doi:10.1007/s00253-014-5646-2
42. Eeckhaut V, Van Immerseel F, Croubels S, De Baere S, Haesebrouck F, Ducatelle R, et al. Butyrate production in phylogenetically diverse Firmicutes isolated from the chicken caecum. Microb Biotechnol (2011) 4(4):503–12. doi:10.1111/j.1751-7915.2010.00244.x
43. De Maesschalck C, Van Immerseel F, Eeckhaut V, De Baere S, Cnockaert M, Croubels S, et al. Faecalicoccus acidiformans gen. nov., sp. nov., isolated from the chicken caecum, and reclassification of Streptococcus pleomorphus (Barnes et al. 1977), Eubacterium biforme (Eggerth 1935) and Eubacterium cylindroides (Cato et al. 1974) as Faecalicoccus pleomorphus comb. nov., Holdemanella biformis gen. nov., comb. nov. and Faecalitalea cylindroides gen. nov., comb. nov., respectively, within the family Erysipelotrichaceae. Int J Syst Evol Microbiol (2014) 64(Pt 11):3877–84. doi:10.1099/ijs.0.064626-0
44. Eeckhaut V, Van Immerseel F, Teirlynck E, Pasmans F, Fievez V, Snauwaert C, et al. Butyricicoccus pullicaecorum gen. nov., sp. nov., an anaerobic, butyrate-producing bacterium isolated from the caecal content of a broiler chicken. Int J Syst Evol Microbiol (2008) 58(Pt 12):2799–802. doi:10.1099/ijs.0.65730-0
45. Eeckhaut V, Van Immerseel F, Pasmans F, De Brandt E, Haesebrouck F, Ducatelle R, et al. Anaerostipes butyraticus sp. nov., an anaerobic, butyrate-producing bacterium from Clostridium cluster XIVa isolated from broiler chicken caecal content, and emended description of the genus Anaerostipes. Int J Syst Evol Microbiol (2010) 60(Pt 5):1108–12. doi:10.1099/ijs.0.015289-0
48. Duncan SH, Louis P, Flint HJ. Lactate-utilizing bacteria, isolated from human feces, that produce butyrate as a major fermentation product. Appl Environ Microbiol (2004) 70(10):5810–7. doi:10.1128/AEM.70.10.5810-5817.2004
49. Louis P, Duncan SH, McCrae SI, Millar J, Jackson MS, Flint HJ. Restricted distribution of the butyrate kinase pathway among butyrate-producing bacteria from the human colon. J Bacteriol (2004) 186(7):2099–106. doi:10.1128/Jb.186.7.2099-2106.2004
51. Belenguer A, Duncan SH, Calder AG, Holtrop G, Louis P, Lobley GE, et al. Two routes of metabolic cross-feeding between Bifidobacterium adolescentis and butyrate-producing anaerobes from the human gut. Appl Environ Microbiol (2006) 72(5):3593–9. doi:10.1128/AEM.72.5.3593-3599.2006
52. El Aidy S, Van den Abbeele P, Van de Wiele T, Louis P, Kleerebezem M. Intestinal colonization: how key microbial players become established in this dynamic process: microbial metabolic activities and the interplay between the host and microbes. Bioessays (2013) 35(10):913–23. doi:10.1002/bies.201300073
55. Marquet P, Duncan SH, Chassard C, Bernalier-Donadille A, Flint HJ. Lactate has the potential to promote hydrogen sulphide formation in the human colon. FEMS Microbiol Lett (2009) 299(2):128–34. doi:10.1111/j.1574-6968.2009.01750.x
57. Hill C, Guarner F, Reid G, Gibson GR, Merenstein DJ, Pot B, et al. Expert consensus document. The international scientific association for probiotics and prebiotics consensus statement on the scope and appropriate use of the term probiotic. Nat Rev Gastroenterol Hepatol (2014) 11(8):506–14. doi:10.1038/nrgastro.2014.66
58. Boesten RJ, de Vos WM. Interactomics in the human intestine: Lactobacilli and Bifidobacteria make a difference. J Clin Gastroenterol (2008) 42(Suppl 3 Pt 2):S163–7. doi:10.1097/MCG.0b013e31817dbd62
59. Kleerebezem M, Vaughan EE. Probiotic and gut Lactobacilli and Bifidobacteria: molecular approaches to study diversity and activity. Annu Rev Microbiol (2009) 63:269–90. doi:10.1146/annurev.micro.091208.073341
64. Fritts CA, Kersey JH, Motl MA, Kroger EC, Yan F, Si J, et al. Bacillus subtilis C-3102 (Calsporin) improves live performance and microbiological status of broiler chickens. J Appl Poult Res (2000) 9(2):149–55. doi:10.1093/japr/9.2.149
65. Stern NJ, Cox NA, Bailey JS, Berrang ME, Musgrove MT. Comparison of mucosal competitive exclusion and competitive exclusion treatment to reduce Salmonella and Campylobacter spp. colonization in broiler chickens. Poult Sci (2001) 80(2):156–60. doi:10.1093/ps/80.2.156
66. Gong J, Si W, Forster RJ, Huang R, Yu H, Yin Y, et al. 16S rRNA gene-based analysis of mucosa-associated bacterial community and phylogeny in the chicken gastrointestinal tracts: from crops to ceca. FEMS Microbiol Ecol (2007) 59(1):147–57. doi:10.1111/j.1574-6941.2006.00193.x
67. Torok VA, Hughes RJ, Mikkelsen LL, Perez-Maldonado R, Balding K, MacAlpine R, et al. Identification and characterization of potential performance-related gut microbiotas in broiler chickens across various feeding trials. Appl Environ Microbiol (2011) 77(17):5868–78. doi:10.1128/AEM.00165-11
70. Hossain MM, Begum M, Kim IH. Effect of Bacillus subtilis, Clostridium butyricum and Lactobacillus acidophilus endospores on growth performance, nutrient digestibility, meat quality, relative organ weight, microbial shedding and excreta noxious gas emission in broilers. Vet Med (2015) 60(2):77–86. doi:10.17221/7981-VETMED
71. Yang CM, Cao GT, Ferket PR, Liu TT, Zhou L, Zhang L, et al. Effects of probiotic, Clostridium butyricum, on growth performance, immune function, and cecal microflora in broiler chickens. Poult Sci (2012) 91(9):2121–9. doi:10.3382/ps.2011-02131
72. Van Immerseel F, Ducatelle R, De Vos M, Boon N, Van De Wiele T, Verbeke K, et al. Butyric acid-producing anaerobic bacteria as a novel probiotic treatment approach for inflammatory bowel disease. J Med Microbiol (2010) 59(2):141–3. doi:10.1099/jmm.0.017541-0
74. Veiga P, Gallini CA, Beal C, Michaud M, Delaney ML, DuBois A, et al. Bifidobacterium animalis subsp. lactis fermented milk product reduces inflammation by altering a niche for colitogenic microbes. Proc Natl Acad Sci U S A (2010) 107(42):18132–7. doi:10.1073/pnas.1011737107
75. Meimandipour A, Shuhaimi M, Hair-Bejo M, Azhar K, Kabeir BM, Rasti B, et al. In vitro fermentation of broiler cecal content: the role of Lactobacilli and pH value on the composition of microbiota and end products fermentation. Lett Appl Microbiol (2009) 49(4):415–20. doi:10.1111/j.1472-765X.2009.02674.x
76. Gibson GR, Probert HM, Loo JV, Rastall RA, Roberfroid MB. Dietary modulation of the human colonic microbiota: updating the concept of prebiotics. Nutr Res Rev (2004) 17(2):259–75. doi:10.1079/NRR200479
77. Kim YJ, Park WY, Choi IH. Effects of dietary alpha-tocopherol, selenium, and their different combinations on growth performance and meat quality of broiler chickens. Poult Sci (2010) 89(3):603–8. doi:10.3382/ps.2009-00280
78. De Maesschalck C, Eeckhaut V, Maertens L, De Lange L, Marchal L, Nezer C, et al. Effects of xylo-oligosaccharides on broiler chicken performance and microbiota. Appl Environ Microbiol (2015) 81(17):5880–8. doi:10.1128/AEM.01616-15
79. Ducatelle R, Eeckhaut V, Haesebrouck F, Van Immerseel F. A review on prebiotics and probiotics for the control of dysbiosis: present status and future perspectives. Animal (2015) 9(1):43–8. doi:10.1017/S1751731114002584
81. Xu ZR, Hu CH, Xia MS, Zhan XA, Wang MQ. Effects of dietary fructooligosaccharide on digestive enzyme activities, intestinal microflora and morphology of male broilers. Poult Sci (2003) 82(6):1030–6. doi:10.1093/ps/82.6.1030
82. Rebole A, Ortiz LT, Rodriguez ML, Alzueta C, Trevino J, Velasco S. Effects of inulin and enzyme complex, individually or in combination, on growth performance, intestinal microflora, cecal fermentation characteristics, and jejunal histomorphology in broiler chickens fed a wheat- and barley-based diet. Poult Sci (2010) 89(2):276–86. doi:10.3382/ps.2009-00336
84. Courtin CM, Swennen K, Broekaert WF, Swennen Q, Buyse J, Decuypere E, et al. Effects of dietary inclusion of xylooligosaccharides, arabinoxylooligoscaccharides and soluble arabinoxylan on the microbial composition of caecal contents of chickens. J Sci Food Agric (2008) 88(14):2517–22. doi:10.1002/jsfa.3373
86. Cao BH, Karasawa Y, Guo YM. Effect of green tea polyphenols and fructo-oligosaccharides in semi-purified diets on broilers’ performance and caecal microflora and their metabolites. AsianAustralas J Anim Sci (2005) 18:85–9. doi:10.5713/ajas.2005.85
87. Fukata T, Sasai K, Miyamoto T, Baba E. Inhibitory effects of competitive exclusion and fructooligosaccharide, singly and in combination, on Salmonella colonization of chicks. J Food Prot (1999) 62(3):229–33.
88. Rehman H, Hellweg P, Taras D, Zentek J. Effects of dietary inulin on the intestinal short chain fatty acids and microbial ecology in broiler chickens as revealed by denaturing gradient gel electrophoresis. Poult Sci (2008) 87(4):783–9. doi:10.3382/ps.2007-00271
Keywords: broiler, endogenous butyrate, performance, probiotics, prebiotics
Citation: Onrust L, Ducatelle R, Van Driessche K, De Maesschalck C, Vermeulen K, Haesebrouck F, Eeckhaut V and Van Immerseel F (2015) Steering Endogenous Butyrate Production in the Intestinal Tract of Broilers as a Tool to Improve Gut Health. Front. Vet. Sci. 2:75. doi: 10.3389/fvets.2015.00075
Received: 05 October 2015; Accepted: 30 November 2015;
Published: 17 December 2015
Edited by:Ryan Arsenault, University of Delaware, USA
Reviewed by:Sherry Layton, Vetanco, Argentina;
Brian B. Oakley, Western University of Health Sciences, USA
Copyright: © 2015 Onrust, Ducatelle, Van Driessche, De Maesschalck, Vermeulen, Haesebrouck, Eeckhaut and Van Immerseel. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Filip Van Immerseel, firstname.lastname@example.org