As an alternative to antibiotic growth promoters, live yeast supplementation has proven useful in reducing weaning stress and improving performance parameters of piglets. Here, we compared the performance and hindgut microbiota of weanling piglets subjected to different pre- and post-weaning yeast supplementation regimens using a live strain of Saccharomyces cerevisiae (Actisaf Sc 47). Average feed intake and average daily weight gain of piglets within Yeast-Control and Yeast-Yeast groups were higher than those in the Control-Control group. Yeast supplementation resulted in development of microbial communities that were phylogenetically more homogenous and less dispersed compared to the microbiota of control piglets. Key bacterial taxa overrepresented in the microbiota of yeast supplemented piglets included phylum Actinobacteria, specifically family Coriobacteriaceae, as well as Firmicutes families Ruminococcaceae, Clostridiaceae, Peptostreptococcaceae, and Peptococcaceae. Correlation network analysis revealed that yeast supplementation was associated with enrichment of positive correlations among proportions of different bacterial genera within the hindgut ecosystem. In particular, within the cecal microbiota of supplemented piglets, higher numbers of positive correlations were observed among potentially beneficial genera of the phyla Actinobacteria and Firmicutes, suggesting a mechanism by which yeast supplementation may contribute to regulation of intestinal homeostasis and improved performance of piglets.
The weaning transition in piglets is a stressful process associated with decreased feed intake, poor performance and increased susceptibility to infection, including post- weaning diarrhea1,2. Antibiotic feed additives have been commonly used during the weaning transition to prevent the post-weaning lag in health and performance of piglets. However, the widespread use of subtherapeutic doses of antibiotics has contributed to the emergence of antibiotic resistant bacteria3, which may be capable of transferring their resistance genes to other pathogenic bacteria of humans and animals4. In addition, the use of antibiotics in animals is becoming a huge concern among consumer groups due to possible drug residues in meat products5. As a result, many countries are banning the inclusion of antibiotics in animal diets. Following the 2006 ban of antibiotic feed additives in Europe and the consumer driven pressure against the use of antibiotics in North America, probiotics are being widely used as an alternative to promote health and performance of farm animals worldwide6,7.
Yeasts have been widely used to promote gut health both in humans8 and animals9. There is considerable evidence showing a positive effect of live yeast, Saccharomyces cerevisiae, supplementation on the health and performance of ruminant animals10. However, data from monogastric animals is still contradictory, some reporting a beneficiary effect of live yeast supplementation on the health and performance of pigs11,12,13,14 and horses15, while others have reported no beneficiary effect of yeast supplementation on the performance of young pigs16,17 or reproductive performance of sows18. Despite few suggested mechanisms8,19, potential modes of action by which live yeast supplementation can improve the overall health and performance of monogastric animals are as yet poorly understood.
The gastrointestinal tract (GIT) of mammals harbors complex microbial communities that provide host animals with a number of protective and metabolic functions including development and modulation of the immune system, extraction and utilization of nutrients from complex indigestible polysaccharides, and competitive exclusion of pathogens20,21,22. Similar to the newborns of other mammalian species, a wide array of biotic and abiotic factors can influence the developmental trajectory of the GIT microbiota of the piglets23. Probiotics have been recognized as biotic factors capable of modulating the symbiotic relationship between host and its GIT microbiota. Some of the proposed mechanisms of actions of probiotics include inhibition of pathogen colonization, stimulation of host’s immune system, and modulation of the composition and functionality of the GIT microbiota24. However, to what extent pre- and post-weaning live yeast supplementation can influence the composition of the GIT microbiota of weanling piglets is poorly understood. In keeping with this, the main objective of the current study was to evaluate the effect of different combinations of pre- and post-weaning S. cerevisiae live yeast supplementation on the growth performance and microbiota profile of the cecal and colonic contents of weanling piglets.
Comparisons of zootechnical data were performed on samples collected from 128 piglets assigned to 4 different treatment groups including Control-Control, Yeast-Control, Control-Yeast and Yeast-Yeast (Supplementary Figure S1). Although the body weight (BW) of piglets belonging to different treatment groups did not differ at the weaning day (P = 0.878), piglets in the Yeast-Yeast group tended (P = 0.074) to be heavier than those in Control-Control and Yeast-Control groups at the end of the experiment. With respect to average daily weight gain (ADG), piglets in the Yeast-Yeast group had higher (P = 0.033) ADG compared to those in Control-Control and Yeast-Control groups. Similarly, piglets in the Control-Yeast group also had significantly higher ADG compared to those in Control-Control group. Pre-weaning yeast supplementation of piglets also improved (P = 0.002) the average daily feed intake (ADFI) of piglets irrespective of whether they received yeast supplementation in the post-weaning period (Yeast-Yeast) or not (Yeast-Control) as compared to piglets that did not receive yeast supplementation at all (Control-Control) or those which received yeast supplementation only during the post-weaning study period (Control-Yeast). Overall, no significant improvement was observed in the performance of piglets when yeast supplementation was started only after weaning (Fig. 1a–d). Furthermore, there was no significant impact of yeast supplementation on the feed conversion ratio (FCR).
As shown in Supplementary Figure S2, both control and treated piglets shed yeast in their feces during the post-weaning period. However, yeast shedding in feces was markedly higher (approximately 2 log cfu/g feces; P < 0.0001) in post-weaning yeast supplemented groups (Yeast-Yeast and Control-Yeast) compared to the control group (Control-Control) or pre-weaning yeast supplementation (Yeast-Control). The same trend was observed in the number of yeast colonies isolated from the cecum contents, where post-weaning yeast supplemented groups had significantly higher (P < 0.0001) yeast counts in their cecal content compared to Control-Control and Yeast-Control groups.
The impact of yeast supplementation on diversity metrics of hindgut microbiota
Microbiota analysis was performed on the cecum (n = 64) and colon (n = 64) contents of piglets slaughtered on day 28 post-weaning (Supplementary Figure S1). On average, 78,752(±21,450) and 91,980(±27,820) high quality sequences were obtained from cecum and proximal colon sample, respectively. These sequences were further clustered into 802 (±113.12) and 998 (±127.07) unique OTUs (at 97% sequence identity) per cecum and proximal colon sample, respectively. Comparison of alpha-diversity indices was performed on rarefied OTU table (even depth of 20,000 OTUs per sample; Supplementary Figure S3). Overall, yeast supplementation did not influence the microbiota richness (observed OTUs and Chao1 estimates of species richness) or diversity (Shannon’s index of diversity and within sample effective counts of Shannon’s index) in either compartments of the GIT. With respect to beta-diversity, PERMANOVA of weighted UniFrac distances revealed that different compartments of the GIT (cecal content vs. colon contents) harbor microbial communities that are phylogenetically distinct from each other (P(PERMANOVA) < 0.001; Fig. 2a). Within the microbiota of both compartments, samples belonging to post-weaning yeast supplemented groups (Yeast-Yeast and Control-Yeast) clustered separately from those belonging to Control-Control and Yeast-Control groups (P(PERMANOVA) < 0.001; Fig. 2b and c). In addition, permutation of dispersions (PERMDISP) of weighted UniFrac distances revealed that cecum contents of piglets assigned to post-weaning yeast supplemented regimens (Yeast-Yeast and Control-Yeast) harbored microbial communities that were phylogenetically more homogenous, and, therefore, less dispersed compared to those belonging to Control-Control and Yeast-Control groups (P(PERMDISP) = 0.005; Fig. 2b). No significant difference was observed between the dispersion of microbial communities of colon contents among treatment groups (P(PERMDISP) = 0.159; Fig. 2c). The impact of experiments (assignment of piglets to different farrowing and nursery rooms of parallel experimental setups) on the overall structure of microbial communities of different compartments of the GIT was also tested revealing a trend (P(PERMANOVA) = 0.068) between the microbiota of colon contents collected form different experimental setups (Supplementary Figure S4). There was no significant interaction (P(PERMANOVA) > 0.1) between the effect of treatment (yeast supplementation regimens) and experimental setups on the microbiota of either niches of the GIT.
Compositional differences among the hindgut microbiota of piglets subjected to different yeast supplementation regimens
Taxonomic classification of representative OTUs resulted in identification of 13 and 15 bacterial phyla in the microbiota of cecum and colon contents, respectively. Within the microbiota of both niches, Firmicutes, followed by Bacteroidetes, Actinobacteria, Proteobacteria, and Spirochaetes were the most dominant phyla (>0.1% of community, Fig. 3). Considerable inter-animal differences existed in the composition of hindgut microbiota of piglets. Overall, Clostridiaceae, Ruminococcaceae, Lactobacillaceae, Lachnospiraceae, and Prevotellaceae were the predominant bacterial families of the hindgut microbiota of piglets, collectively accounting for more than 70% of the bacterial communities within both cecum and colon contents (Supplementary Figure S5).
At the phylum level, the proportion of Actinobacteria was significantly (P < 0.05) higher in the microbiota of cecum and colon contents of piglets assigned to pre- and post-weaning yeast supplementation regimens (Yeast-Yeast) than those in the Control-Control or Yeast-Control groups (Fig. 3). In line with the results of PERMANOVA, statistical comparisons at lower taxonomic levels (family, genus and OTU) were focused on comparisons between the two treatment groups that harbored most distinct microbiota profiles (i.e. Control-Control versus Yeast-Yeast; Tables 1 and 2). Proportions of actinobacterial family Coriobacteriaceae, as well as Firmicutes families Halanaerobiaceae, Peptococcaceae, Peptostreptococcaceae, Ruminococcaceae, and Turicibacteraceae were significantly (q < 0.05) higher in the microbiota of cecum and colon contents of piglets receiving the Yeast-Yeast supplementation regimen than Control-Control. These significant associations were further traced back to overrepresentations of several OTUs in the hindgut microbiota of Yeast-Yeast supplemented piglets, including those assigned to genera Collinsella, Peptococcus, Ruminococcus, Turicibacter. In addition, OTUs belonging to the genus Mitsuokella, within the family Veillonellaceae, were also significantly higher in the microbiota of Yeast-Yeast supplemented piglets. On the other hand, within the microbiota of both niches, Firmicutes OTUs belonging to Lactobacillus and Bacteroidetes OTUs belonging to Prevotella were overrepresented within the microbiota of piglets receiving the Control-Control regimen.
Correlation of hindgut microbiota with performance parameters and yeast cell count in luminal contents
Spearman’s rank correlation coefficient (rho) was used to explore the relationship of bacterial taxa at family and genus levels with ADG and FCR (Supplementary Figure S6). In the microbiota of cecum contents, genus Mitsuokella was positively correlated with ADG (rho = 0.303; P = 0.016), whereas an unclassified genus within the family Veillonellaceae was negatively correlated with ADG (rho = −0.301; P = 0.017). Within the microbiota of colon contents, Mitsuokella showed positive correlations with both ADG (rho = 0.279; P = 0.038) and FCR (rho = 0.368; P = 0.006). Clostridiales genus Mogibacterium was also positively correlated with ADG (rho = 0.432; P = 0.001).
MaAsLin was further used to explore potential associations between bacterial taxa and log10 yeast cell count (cfu/g) in luminal content (Tables 1 and 2). Within the microbiota of cecum contents, significant positive associations were observed between yeast cell count and the proportions of families Halanaerobiaceae and Peptostreptococcaceae. Similarly, bacterial OTUs belonging to families Clostridiaceae and Peptostreptococcaceae were also positively associated with the abundance of yeast in the cecum contents. On the other hand, the proportion of unclassified Bacteroidales was negatively associated with yeast cell count of the cecum contents. Within the colon microbiota, the proportions of the family Peptococcaceae, as well as OTUs belonging to genus Collinsella and family Peptostreptococcaceae were positively associated with yeast cell count in colon contents.
Yeast supplementation alters the co-occurrence pattern of hindgut microbiota
Comparison of the correlation patterns of bacterial genera (i.e. positive correlations suggestive of co-occurrence and negative correlations suggestive of mutual exclusion) provided further insights into the impact of yeast supplementation on the overall structures of cecum and colon microbial communities. In the cecum microbiota, yeast supplementation (represented by Yeast-Yeast group) decreased the total number of negative correlations among proportions of different bacterial genera and therefore, compared to the Control-Control group, increased the ratio of positive-edges over negative ones (2.31 vs. 0.99, respectively; Supplementary Table S1). A closer look at the profile of hub bacterial genera (genera showing the highest number of significant positive and/or negative correlations with other members of the community) revealed that in the cecum microbiota of Control-Control piglets, genera Lactobacillus, Megasphaera, and Bacteroides had the highest number of connections (mostly mutual exclusion) with the rest of the community, whereas in the microbiota of Yeast-Yeast supplemented piglets, genera Dorea and Faecalibacterium, along with unclassified Halanaerobiaceae and Clostridiales had the highest number of connections (mostly co-occurrence relationships) within the community. In addition, in the cecum microbiota of Yeast-Yeast supplemented piglets, actinobacterial genera Collinsella and unclassified Coriobacteriaceae also showed increased connectivity (co-occurrence relationships) with other members of the community (Fig. 4a and b). On the other hand, in the microbiota of colon contents, the ratio of positive-edges over negative ones remained roughly stable between the two groups of piglets (1.13 vs. 1.18, in Yeast-Yeast vs. Control-Control groups, respectively; Supplementary Table S1). Nonetheless, the profile of hub genera was different between the microbiota of the two groups; Lactobacillus and Megasphaera were the most connected (mutual exclusion relationships) genera within the colon microbiota of Control-Control piglets, whereas in the microbiota of Yeast-Yeast supplemented piglets, genera Bacteroides and unclassified Bacteroidales, along with unclassified Enterobacteriaceae were the most connected (mutual exclusion relationships) members of the community (Fig. 5a and b).
Finally, the relative degree of connectance of bacterial phyla (i.e. the total number of significant correlations of bacterial genera belonging to each phylum divided by the average proportion of that phylum) was measured to assess the impact of yeast supplementation on the influential capacity of main bacterial phyla within the microbiota of cecum and colon contents. In general, irrespective of treatment groups and GIT niche, the relative contributions of less dominant bacterial phyla including Actinobacteria, Proteobacteria and Spirochaetes were higher than those of the predominant bacterial phyla Firmicutes and Bacteroidetes. Overall, with the exception of Bacteroidetes, yeast supplementation was associated with reduced negative connectance of all bacterial phyla within the microbiota of cecum content. On the other hand, in the microbiota of colon contents, the relative degrees of negative connectance of Bacteroidetes and Spirochaetes were increased by yeast supplementation. Within the microbiota of both niches, yeast supplementation increased the positive connectance of Actinobacteria (Fig. 6a and b).
Here, we described the impact of different combinations of pre- and post-weaning live yeast supplementation on the growth performance and hindgut microbiota profiles of weanling piglets. Our results indicated that pre-weaning yeast supplementation, irrespective of provision of yeast supplementation during the post-weaning period, improved the performance parameters of the weanling piglets, whereas yeast supplementation provided only during the post-weaning period failed to improve the performance of piglets. On the other hand, the effect of yeast on the composition of hindgut microbiota was more pronounced when provided during the post-weaning period, with the most distinct microbial communities belonging to the piglets that received yeast supplementation both pre- and post-weaning. The microbiota of this group of piglets were phylogenetically more homogenous than those of the control piglets, showing an increased ratio of positive correlations over negative ones; a pattern typical of cooperative microbial ecosystems that are mainly composed of non-competing species25. By using a combination of correlation network analysis and multivariate associative tests, we further identified key bacterial taxa that were central to the structure of hindgut microbiota profile of yeast-supplemented piglets.
In the present study, piglets supplemented with yeast during the pre-weaning period had significantly higher ADG and ADFI than their counterparts in the Control-Control and Control-Yeast groups. This implies that pre-weaning live yeast supplementation, even in the absence of post-weaning supplementation, can improve the performance of weaned piglets in the nursery. In contrast to previous reports11,13,14, our results indicated that yeast supplementation only during the post-weaning period did not improve the performance of piglets. Positive effects of yeast supplementation may be partly due to the ability of yeast to modify the composition of gut microbiota26 and/or enhance the immune responsiveness of the piglets27,28 early in life. In other words, yeast supplementation may be able to regulate intestinal homeostasis during early stages of life and therefore alleviate the negative effects of weaning-associated stress and its consequent metabolic disorders such as diarrhea. Our results suggested that yeast supplementation only during the post-weaning period could be “too little too late” to exert positive effect during the weaning transition and make an impact on the performance of weaned piglets. Nonetheless, only piglets in the Yeast-Yeast group weighted significantly heavier than the control group at the end of the study period, indicating the superiority of continuous pre- and post-weaning supplementation of live yeast over other supplementation regimens. In agreement with this, Trckova and colleagues27 showed that dietary supplementation with live yeast (S. cerevisiae) in sows during the late gestation, and in piglets during the suckling and post-weaning periods, resulted in increased plasma levels of IgA, reduced the duration and severity of post-weaning diarrhea, and consequently improved production and performance of weaned piglets. Therefore, it appears that in order to achieve optimum beneficial impacts on the production and performance parameters, yeast supplementation needs to be provided to piglets during both suckling and nursery periods. Under commercial farm settings, however, mechanical feeding of piglets with yeast is impractical. Alternatively, yeast can be supplemented to sows during the late gestation and early suckling period, which will act as a potential source of yeast to piglets through shedding of live yeast in the sow feces. During this period, yeast-induced immunoglobulin may also be transferred vertically from supplemented sows to the suckling piglets.
As indicated earlier, potential mechanisms by which yeast supplementation can modulate the performance of piglets are as yet poorly understood. In contrast to previous reports regarding the inability of live yeast supplementation in modifying the gut microbiota of weanling piglets11,14, we and others29 suggest that improved performance of yeast supplemented piglets can be partly due to the influence of live yeast on the composition of the hindgut microbiota. During the first few weeks of life, the gut microbiota of piglets are reported to be unstable and prone to modification30,31. Therefore, live yeast supplementation to piglets during early stages of life may have the highest potential to modify the composition and functionality of the gut microbiota. In the present study, we did not observe any significant difference among the indices of species-richness and α-diversity of the hindgut microbiota of piglets assigned to different treatment groups. Nonetheless, yeast supplementation, particularly during the post-weaning period, modified the composition and structure of the microbiota of both cecum and colon contents. In conjunction with evaluating the phylogenetic distance and dispersion of microbial communities, correlation network analysis has the potential to convey important information about the structural features of microbial communities and driving forces behind them32,33. In the present work, pair-wise comparisons of UniFrac distances between treatment groups indicated that cecum and colon content of yeast supplemented piglets harbored microbial communities that were more homogenous (i.e. phylogenetically less disperse). From an ecological perspective, phylogenetic dispersion of microbial communities can be a sign of strong negative relationships between competing species that thrive on similar nutrient resources25,34. In the present study, evaluation of co-occurrence patterns among the proportion of different bacterial genera revealed that yeast supplementation increased the ratio of positive/negative connections within the microbiota of cecum contents, resulting in development of microbial communities that were phylogenetically more homogenous than those of the control piglets. This was on one hand achieved by suppressing negative correlations of spirochaetal and proteobacterial genera with the rest of the community, and on the other hand by promoting the positive connections of several actinobacterial and Firmicutes genera. Enrichment of positive feedbacks within a microbial community can be roughly translated to the presence of microbial species that benefit from the metabolic activity of each other (i.e. mutualistic interactions). Such communities can therefore effectively utilize available nutrient resources within the ecosystem and prevent colonization by opportunistic and/or pathogenic species35. Our correlation network analysis revealed that within the microbiota of cecum contents, yeast supplementation resulted in increased number of positive correlations of actinobacterial and Firmicutes genera with other members of the community. Compared to Firmicutes and Bacteroidetes, Actinobacteria represent a lower proportion of the GIT microbiota in mammals. This is to some extent due to underestimation of the real proportion of this phylum by PCR-based 16 S rRNA gene sequencing approaches36. Despite this artifact, due to the relatively large impact that actinobacterial genera usually have on the overall structure of the microbial community, members of this phylum have been nominated as “keystone taxa” that can play substantial role in modulating the functionality of the GIT microbiome33.
In the present study, in addition to increased connectivity of actinobacterial genera, we observed an overall increase in the proportion of phylum Actinobacteria in response to yeast supplementation. At the genus level, actinobacterial genera Bifidobacterium and Collinsella were enriched in the microbiota of cecum and proximal colon of yeast supplemented piglets. Both of these bacterial genera have been associated with beneficial health effects; Bifidobacterium spp. have been extensively used as probiotic37 known to possess competing activities against pathogens via several mechanisms38. Decreased proportion of Collinsella spp. has been associated with development of dysbiotic gut microbiota in inflammatory bowel disease (IBD)39. Under poor environmental hygiene and/or during stressful times such as weaning, the mannan oligosaccharides (MOS) component of yeast cell wall can favor the growth of beneficial bacteria, such as Bifidobacteria and Lactobacilli, in the hindgut while reducing the number of pathogenic E. coli and Salmonella40. Concomitant with increased proportion of Bifidobacterium, we observed a decline in the proportion of Lactobacillus, particularly in the cecum microbiota. Others13,26 have also reported decreased proportion of Lactobacillus in the hindgut microbiota of pigs in response to yeast supplementation. As suggested by Martin et al.41, this observation might be indicative of competition between Bifidobacteria and Lactobacilli over yeast-derived changes in the profile of hindgut metabolite.
Beside the proposed role of Actinobacteria in modulating the piglets’ gut microbiota following yeast supplementation, the proportions of several potentially beneficial bacteria within the phylum Firmicutes were also increased in the microbiota of cecum and colon contents of yeast-supplemented piglets. This included, among others, increase in the proportion of family Ruminococcaceae, which include major fiber degrading and butyrate producing bacteria42, and genus Mitsuokella, which has been previously reported to inhibit the growth of Salmonella enterica serovar Typhimurium in pigs43. In addition, we observed that Mitsuokella was also positively correlated with performance parameters such as ADG and FCR. Taking all these together, one can suggest that yeast supplementation to neonatal piglets modifies the hindgut microbiota of weanling piglets towards a healthy balance by promoting positive relationships among beneficiary bacteria while suppressing the competitiveness and proportion of potentially harmful bacterial populations.
In conclusion, our results showed that live yeast supplementations during the pre-weaning period enhanced pig performance post-weaning in the nursery and this effect is prominent and statistically significant when yeast supplementation is continued post-weaning in the nursery. Interestingly, we identified several shifts in the composition of the hindgut microbiota that were associated with improved performance parameters of the yeast-supplemented piglets. In particular, yeast supplementation tended to modify the structure of the hindgut microbiota towards a phylogenetically more homogenous profile, enriched with positive interaction among potentially beneficial members of the phyla Actinobacteria and Firmicutes.
The two animal studies were conducted according to the regulations and guidelines provided by the Canadian Council on Animal Care (CCAC) for humane animal use and approved by the University of Saskatchewan Animal Research Ethics Board (AREB) under animal use protocol number AUP-20110132.
Eight sows with their newborn piglets were selected among the farrowing sows at the prairie swine center and randomly assigned to two groups (Yeast vs. Control) with 4 sows in each group placed in farrowing crates on opposite sides of the same room. Eight piglets, balanced for gender and body weight (≥800 g), were selected from each sow and ear tagged for identification. Piglets from the 4 sows in the Yeast group (n = 32) received a solution containing ~2.5 × 1010 cfu of live Saccharomyces cerevisiae yeast (Actisaf, CNCM I-4407, Phileo Lesaffre Animal Care, France) per pig by oral gavage every other day starting from day 1 of age until weaning (Yeast group). Similarly, piglets from the remaining 4 control sows on the opposite side of the room (n = 32) were treated with equal volume of sterile water (Control group). Piglets were weaned at 26.6 ± 0.74 days of age to a cereal based diet shown on Supplementary Table S2. During the post-weaning period, 16 piglets from the Control group and 16 piglets from the Yeast group received diet without yeast and another 16 piglets from each group received yeast-supplemented diet containing 107 cfu of live yeast per gram of dry pelleted feed (Yeast diet). Therefore, during the post-weaning period we had 4 treatment groups including Control-Control, Yeast-Control, Control-Yeast and Yeast-Yeast groups. Due to space limitation, a parallel experiment with identical number of piglets and experimental setups was performed in separate farrowing and nursery rooms. Details of the study design, including the treatment groups, number of pens per treatment, as well as number of pigs per pen are schematically represented in the Supplementary Figure S1.
Piglets’ body weight (BW) was taken every week starting immediately after birth (between day1 to 3 of age) until weaning to determine average daily gain (ADG) for the pre-weaning period. After weaning, feed consumption and piglet weights were collected every week to determine feed conversion rate and ADG for the post weaning growth phase. Fecal sample was also collected once a week to determine the fecal shedding of yeast in the different groups of pigs. Four weeks after weaning, 2 pigs per pen, 8 pigs per treatment group (n = 32 for experiment 1 and n = 32 for experiment 2) were humanely killed by captive bolt stunning and pithing to permit collection of hindgut contents for culture and microbial ecology studies. Fecal and intestinal content samples were serially diluted in peptone water and plated (100ul /plate) on YGC agar plates (Sigma-Aldrich, St. Louise, MO, USA) to determine yeast load per gram of cecum or colon content both in the yeast treated and control piglets. Yeast cell counts in pelleted feed samples were also monitored by plating serially diluted feed samples on YGC agar plates to ensure that yeast cells survived the pelleting temperature.
DNA extraction and sequencing
Total genomic DNA was extracted from 350 mg intestinal content samples by bead-beating method using the 25:24:1 phenol/chloroform/isoamyl alcohol extraction technique as previously described44. DNA samples extracted from cecum and proximal colon contents were subjected to deep sequence analysis at MR DNA (www.mrdnalab.com, Shallowater, TX, USA) using the universal Eubacterial primers 27 F (AGRGTTTGATCMTGGCTCAG) and 519 R (GTNTTACNGCGGCKGCTG) to target the V1-V3 regions of 16 S rRNA gene. Amplification was performed in a 30 cycle PCR using the HotStarTaq Plus Master Mix Kit (Qiagen, Valencia, CA, USA) under the following conditions: 94 °C for 3 min followed by 28 cycles of 94 °C for 30 s, 53 °C for 40 s and 72 °C for 1 min, after which a final elongation step at 72 °C for 5 min was performed. Pooled and purified PCR products were used to prepare DNA library following Illumina TruSeq DNA library preparation protocol. Sequencing was performed on a MiSeq following the manufacturer’s guidelines. The sequencing data are uploaded into the Sequence Read Archive (SRA) of NCBI (http://www.ncbi.nlm.nih.gov/sra) and can be accessed through accession number SRR5515885. Metadata file used for processing the sequencing data and conducting statistical analyses can be found in Supplementary Table S3.
The FLASH assembler (v. 1.2.11)45 was used to merge overlapping paired-end Illumina fastq files. The output fastq file was then analyzed using QIIME v.1.846. Chimeric reads were filtered using UCHIME47 and sequences were assigned to Operational Taxonomic Units (OTUs) using the QIIME implementation of UCLUST48 at 97% pairwise identity threshold. An even depth of 20,000 sequences per sample was used for calculation of richness (observed OTUs and Chao1 estimates of species richness) or diversity (Shannon’s index of diversity) indices for cecum and proximal colon samples. Within-sample true diversity (effective counts of Shannon’s index) was calculated according to Jost49. β-diversity of microbial communities was calculated based on weighted UniFrac distances50 and principal coordinate analysis (PCoA) was applied on resulting distance matrices to generate two-dimensional plots using the online package MicrobiomeAnalyst51.
The UNIVARIATE procedure of SAS (SAS 9.3; SAS Institute Inc., Cary, NC, USA) was used to test the normality of residuals for zootechnical data, alpha-diversity indices, and relative abundances of main bacteria phyla. Non-normally distributed data were subjected to log transformation and then used to assess the effect of yeast supplementation on each variable. All pairwise comparisons among the treatment groups were tested using Tukey’s studentized range adjustment, and statistical significance was defined at P < 0.05. Trends were discussed at P < 0.10. Permutational multivariate analysis of variance (PERMANOVA; implemented in PRIMER-6 software, PRIMER-E Ltd, Plymouth Marine Laboratory) was used to detect significant differences between β-diversity measures of microbial communities. Permutation of dispersions (PERMDISP) was also used in parallel to test the homogeneity of dispersions (compare the distances of observations to their group centroids52). Multivariate analysis with linear modeling (MaAsLin)53 was used to determine significant associations of bacterial taxa at different taxonomic levels (family, genus, and OTU) with yeast supplementation (comparisons made between Control-Control and Yeast-Yeast groups) and Log10 yeast cell count (cfu/g of cecum or colon content). MaAsLin included a general linear model with treatment group (2 levels) and experiment (2 levels) as categorical predictor variable, yeast cell count as continuous predictor variable, and arcsin-square root transformed abundances of bacterial taxa at taxonomic levels as the response variable. Multiple hypotheses were adjusted by Benjamini and Hockberg false discovery rate (FDR) and significant associations were considered below a q-value threshold of 0.1.
Correlation network analysis (CoNet54) was used to evaluate the impact of yeast supplementation on the co-occurrence pattern of cecum and colon microbial communities (comparison made between control-control and yeast-yeast groups). In this ensemble method, a combination of diverse measures of correlation (including Pearson’s and Spearman’s correlation coefficients) and dissimilarity (Bray-Curtis and Kullback-Leibler dissimilarities) were used to overcome major challenges in the inference of co-occurrence networks, particularly those introduced by sparse (zero-inflated) data, compositionality, and determination of statistical significance. In brief, for each measure, distributions of all pair-wise scores between the nodes (that are the relative abundances of genera present in >75% of the samples) were computed. For each measure and edge (that is positive or negative correlation between two nodes), 500 permutations were conducted (including renormalization step for Pearson and Spearman measures). Measure-specific p-values were then merged using Brown’s method and after applying Benjamini–Hochberg’s false discovery rate (FDR) correction, only edges with merged p-values below 0.05 and those supported by at least 3 of the abovementioned measures were kept in the final networks. Hub genera were defined as those showing the highest number of positive and/or negative connection (significant co-occurrence and mutual exclusion relationships, respectively) with other members of the community. The relative degree of connectance of main bacterial phyla, a measure used to examine the influential capacity of bacterial taxa33, was calculated based on the total number of positive and negative edges belonging to bacterial genera within each phylum divided by mean relative abundance of that phylum within the community.
Campbell, J. M., Crenshaw, J. D. & Polo, J. The biological stress of early weaned piglets. J. Anim. Sci. Biotechnol. 4, 19, https://doi.org/10.1186/2049-1891-4-19 (2013).
Heo, J. M. et al. Gastrointestinal health and function in weaned pigs: a review of feeding strategies to control post-weaning diarrhoea without using in-feed antimicrobial compounds. J. Anim. Physiol. Anim. Nutr. 97, 207–237, https://doi.org/10.1111/j.1439-0396.2012.01284.x (2013).
Smith, M. G. et al. Antimicrobial resistance and virulence gene profiles in multi-drug resistant enterotoxigenic Escherichia coli isolated from pigs with post-weaning diarrhoea. Vet. Microbiol. 145, 299–307, https://doi.org/10.1016/j.vetmic.2010.04.004 (2010).
Marshall, B. M. & Levy, S. B. Food animals and antimicrobials: impacts on human health. Clin. Microbiol. Rev. 24, 718–733, https://doi.org/10.1128/CMR.00002-11 (2011).
Lusk, J. L., Norwood, F. B. & Pruitt, J. R. Consumer demand for a ban on antibiotic drug use in pork production. Am. J. Agric. Econ. 88, 1015–1033, https://doi.org/10.1111/j.1467-8276.2006.00913.x (2006).
Kenny, M., Smidt, H., Mengheri, E. & Miller, B. Probiotics - do they have a role in the pig industry? Animal. 5, 462–470, https://doi.org/10.1017/S175173111000193X (2011).
Cheng, G. Y. et al. Antibiotic alternatives: the substitution of antibiotics in animal husbandry? Front. Microbiol. 5, https://doi.org/10.3389/Fmicb.2014.00217 (2014).
Czerucka, D., Piche, T. & Rampal, P. Yeast as probiotics - Saccharomyces boulardii. Aliment. Pharmacol. Ther. 26, 767–778, https://doi.org/10.1111/j.1365-2036.2007.03442.x (2007).
Chaucheyras-Durand, F. & Durand, H. Probiotics in animal nutrition and health. Benef. Microbes 1, 3–9, https://doi.org/10.3920/BM2008.1002 (2010).
Desnoyers, M., Giger-Reverdin, S., Bertin, G., Duvaux-Ponter, C. & Sauvant, D. Meta-analysis of the influence of Saccharomyces cerevisiae supplementation on ruminal parameters and milk production of ruminants. J. Dairy Sci. 92, 1620–1632, https://doi.org/10.3168/jds.2008-1414 (2009).
Mathew, A. G., Chattin, S. E., Robbins, C. M. & Golden, D. A. Effects of a direct-fed yeast culture on enteric microbial populations, fermentation acids, and performance of weanling pigs. J. Anim. Sci. 76, 2138–2145, https://doi.org/10.2527/1998.7682138x (1998).
Van der Peet-Schwering, C. M., Jansman, A. J., Smidt, H. & Yoon, I. Effects of yeast culture on performance, gut integrity, and blood cell composition of weanling pigs. J. Anim Sci 85, 3099–3109, https://doi.org/10.2527/jas.2007-0110 (2007).
Van Heugten, E., Funderburke, D. W. & Dorton, K. L. Growth performance, nutrient digestibility, and fecal microflora in weanling pigs fed live yeast. J. Anim. Sci. 81, 1004–1012, https://doi.org/10.2527/2003.8141004x (2003).
Li, J. Y. et al. Effects of live yeast on the performance, nutrient digestibility, gastrointestinal microbiota and concentration of volatile fatty acids in weanling pigs. Arch. Anim. Nutr. 60, 277–288, https://doi.org/10.1080/17450390600785343 (2006).
Medina, B., Girard, I. D., Jacotot, E. & Julliand, V. Effect of a preparation of Saccharomyces cerevisiae on microbial profiles and fermentation patterns in the large intestine of horses fed a high fiber or a high starch diet. J. Anim. Sci. 80, 2600–2609, https://doi.org/10.2527/2002.80102600x (2002).
Kornegay, E. T., Rheinwelker, D., Lindemann, M. D. & Wood, C. M. Performance and Nutrient Digestibility in Weanling Pigs as Influenced by Yeast Culture Additions to Starter Diets Containing Dried Whey or One of 2 Fiber Sources. J. Anim. Sci. 73, 1381–1389, https://doi.org/10.2527/1995.7351381x (1995).
Veum, T. L. & Bowman, G. L. Sacharomyces Cervisiae Yeast Culture in Diets for Mechanically-Fed Neonatal Piglets and Early Growing Self-Fed Pigs. J. Anim. Sci. 37, 67–71, https://doi.org/10.2527/jas1973.37167x (1973).
Veum, T. L., Reyes, J. & Ellersieck, M. Effect of Supplemental Yeast Culture in Sow Gestation and Lactation Diets on Apparent Nutrient Digestibilities and Reproductive-Performance through One Reproductive-Cycle. J. Anim. Sci. 73, 1741–1745, https://doi.org/10.2527/1995.7361741x (1995).
Auclair, E. In Feed manufacturing in the Mediterranean region. Improving safety: From feed to food. (ed J. Bru fau) 45–53 (Cahiers Options Méditerranéennes; n. 54, 2001).
Ley, R. E., Lozupone, C. A., Hamady, M., Knight, R. & Gordon, J. I. Worlds within worlds: evolution of the vertebrate gut microbiota. Nature reviews. Microbiology 6, 776–788, https://doi.org/10.1038/nrmicro1978 (2008).
Neish, A. S. Mucosal immunity and the microbiome. Ann. Am. Thorac. Soc. 11(Suppl 1), S28–32, https://doi.org/10.1513/AnnalsATS.201306-161MG (2014).
Trompette, A. et al. Gut microbiota metabolism of dietary fiber influences allergic airway disease and hematopoiesis. Nat. Med. 20, 159–166, https://doi.org/10.1038/nm.3444 (2014).
Kim, H. B. & Isaacson, R. E. The pig gut microbial diversity: Understanding the pig gut microbial ecology through the next generation high throughput sequencing. Vet. Microbiol. 177, 242–251, https://doi.org/10.1016/j.vetmic.2015.03.014 (2015).
Ng, S., Hart, A., Kamm, M., Stagg, A. & Knight, S. Mechanisms of action of probiotics: recent advances. Inflamm. Bowel. Dis. 15, 300–310, https://doi.org/10.1002/ibd.20602 (2009).
Nemergut, D. R. et al. Patterns and processes of microbial community assembly. Microbiol. Mol. Biol. Rev. 77, 342–356, https://doi.org/10.1128/MMBR.00051-12 (2013).
Upadrasta, A. et al. The Effect of Dietary Supplementation with Spent Cider Yeast on the Swine Distal Gut Microbiome. PloS one 8, https://doi.org/10.1371/journal.pone.0075714 (2013).
Trckova, M. et al. The effects of live yeast Saccharomyces cerevisiae on postweaning diarrhea, immune response, and growth performance in weaned piglets. J. Anim. Sci. 92, 767–774, https://doi.org/10.2527/jas.2013-6793 (2014).
Trevisi, P. et al. Comparison of three patterns of feed supplementation with live Saccharomyces cerevisiae yeast on postweaning diarrhea, health status, and blood metabolic profile of susceptible weaning pigs orally challenged with Escherichia coli F4ac. J. Anim. Sci. 93, 2225–2233, https://doi.org/10.2527/jas.2014-8539 (2015).
Price, K. L. et al. Use of Saccharomyces cerevisiae fermentation product on growth performance and microbiota of weaned pigs during Salmonella infection. J. Anim. Sci. 88, 3896–3908, https://doi.org/10.2527/jas.2009-2728 (2010).
Petri, D., Hill, J. & Van Kessel, A. Microbial succession in the gastrointestinal tract (GIT) of the preweaned pig. Livest. Sci. 133, 107–109, https://doi.org/10.1016/j.livsci.2010.06.037 (2010).
Thompson, C. L., Wang, B. & Holmes, A. J. The immediate environment during postnatal development has long-term impact on gut community structure in pigs. ISME J. 2, 739–748, https://doi.org/10.1038/ismej.2008.29 (2008).
Levy, R. & Borenstein, E. Metabolic modeling of species interaction in the human microbiome elucidates community-level assembly rules. PNAS 110, 12804–12809, https://doi.org/10.1073/pnas.1300926110 (2013).
Trosvik, P. & Muinck, E. J. Ecology of bacteria in the human gastrointestinal tract—identification of keystone and foundation taxa. Microbiome 3, 1, https://doi.org/10.1186/s40168-015-0107-4 (2015).
Weiher, E. & Keddy, P. A. Assembly rules, null models, and trait dispersion: new questions from old patterns. Oikos, 159–164, https://doi.org/10.2307/3545686 (1995).
Stachowicz, J. J. Mutualism Facilitation, and the Structure of Ecological Communities. Positive interactions play a critical, but underappreciated, role in ecological communities by reducing physical or biotic stresses in existing habitats and by creating new habitats on which many species depend. Bioscience 51, 235–246, https://doi.org/10.1641/0006-3568(2001)051[0235:MFATSO]2.0.CO;2 (2001).
Zhernakova, A. et al. Population-based metagenomics analysis reveals markers for gut microbiome composition and diversity. Science 352, 565–569, https://doi.org/10.1126/science.aad3369 (2016).
Druart, C., Alligier, M., Salazar, N., Neyrinck, A. M. & Delzenne, N. M. Modulation of the gut microbiota by nutrients with prebiotic and probiotic properties. Adv. Nutr. 5, 624S–633S, https://doi.org/10.3945/an.114.005835 (2014).
Boesten, R. J. & de Vos, W. M. Interactomics in the human intestine: Lactobacilli and Bifidobacteria make a difference. J. Clin. Gastroenterol. 42, S163–S167, https://doi.org/10.1097/MCG.0b013e31817dbd62 (2008).
Kassinen, A. et al. The Fecal Microbiota of Irritable Bowel Syndrome Patients Differs Significantly From That of Healthy Subjects. Gastroenterology 133, 24–33, https://doi.org/10.1053/j.gastro.2007.04.005 (2007).
Halas, V. & Nochta, I. Mannan oligosaccharides in nursery pig nutrition and their potential mode of action. Animals 2, 261–274 (2012).
Martin, F. P. et al. Top-down systems biology integration of conditional prebiotic modulated transgenomic interactions in a humanized microbiome mouse model. Mol. Syst. Biol. 4, 205, https://doi.org/10.1038/msb.2008.40 (2008).
Cheng, K. J., Forsberg, C. W., Minato, H. & Costerton, J. W. Microbial Ecology and Physiology of Feed Degradation within the Rumen. Physiological Aspects of Digestion and Metabolism in Ruminants, 595–624, https://doi.org/10.1016/B978-0-12-702290-1.50031-X (1991).
Levine, U. Y., Bearson, S. M. & Stanton, T. B. Mitsuokella jalaludinii inhibits growth of Salmonella enterica serovar Typhimurium. Vet. Microbiol. 159, 115–122, https://doi.org/10.1016/j.vetmic.2012.03.027 (2012).
Dumonceaux, T. J. et al. Enumeration of specific bacterial populations in complex intestinal communities using quantitative PCR based on the chaperonin-60 target. J. Microbiol. Methods. 64, 46–62, https://doi.org/10.1016/j.mimet.2005.04.006 (2006).
Magoc, T. & Salzberg, S. L. FLASH: fast length adjustment of short reads to improve genome assemblies. Bioinformatics 27, 2957–2963, https://doi.org/10.1093/bioinformatics/btr507 (2011).
Caporaso, J. G. et al. QIIME allows analysis of high-throughput community sequencing data. Nat. Methods 7, 335–336, https://doi.org/10.1038/nmeth.f.303 (2010).
Edgar, R. C., Haas, B. J., Clemente, J. C., Quince, C. & Knight, R. UCHIME improves sensitivity and speed of chimera detection. Bioinformatics 27, 2194–2200, https://doi.org/10.1093/bioinformatics/btr381 (2011).
Edgar, R. C. Search and clustering orders of magnitude faster than BLAST. Bioinformatics 26, 2460–2461, https://doi.org/10.1093/bioinformatics/btq461 (2010).
Jost, L. Entropy and diversity. Oikos 113, 363–375 (2006).
Lozupone, C. & Knight, R. UniFrac: a new phylogenetic method for comparing microbial communities. Appl. Environ. Microbiol. 71, 8228–8235, https://doi.org/10.1128/AEM.71.12.8228-8235.2005 (2005).
Dhariwal, A. et al. MicrobiomeAnalyst: a web-based tool for comprehensive statistical, visual and meta-analysis of microbiome data. Nucleic. Acids. Res., https://doi.org/10.1093/nar/gkx295 (2017).
Anderson, M. J. & Walsh, D. C. PERMANOVA, ANOSIM, and the Mantel test in the face of heterogeneous dispersions: what null hypothesis are you testing? Ecol. Monogr. 83, 557–574, https://doi.org/10.1890/12-2010.1 (2013).
Morgan, X. C. et al. Dysfunction of the intestinal microbiome in inflammatory bowel disease and treatment. Genome Biol. 13, R79, https://doi.org/10.1186/gb-2012-13-9-r79 (2012).
Faust, K. et al. Microbial co-occurrence relationships in the human microbiome. PLoS Comput. Biol. 8, e1002606, https://doi.org/10.1371/journal.pcbi.1002606 (2012).
The authors would like to express their appreciation to all staff at the Prairie Swine Center Inc., especially, Mr. Brian Andries (Manger-Operations) and Dr. Denise Beaulieu (Research Scientist) for facilitating all our animal experiments.
This project is funded by the Phileo-Lesaffre Animal Care, Lesaffre group France. Co-authors RD‡ and EA‡ are employees of Phileo-Lesaffre Animal Care, the company who funded the study.
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Kiros, T.G., Derakhshani, H., Pinloche, E. et al. Effect of live yeast Saccharomyces cerevisiae (Actisaf Sc 47) supplementation on the performance and hindgut microbiota composition of weanling pigs. Sci Rep 8, 5315 (2018). https://doi.org/10.1038/s41598-018-23373-8
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