Skip to main content
PMC home page
Frontiers in Nutrition logoLink to Frontiers in Nutrition
. 2021 Jul 9;8:686053. doi: 10.3389/fnut.2021.686053

The Enhancement of Intestinal Immunity in Offspring Piglets by Maternal Probiotic or Synbiotic Supplementation Is Associated With the Alteration of Gut Microbiota

Kai Wang 1,2, Chengjun Hu 1, Wu Tang 1, Md Abul Kalam Azad 1, Qian Zhu 1, Qinghua He 2, Xiangfeng Kong 1,*
PMCID: PMC8298840  PMID: 34307437

Abstract

A total of 64 pregnant Bama mini-pigs were used to investigate the effects of maternal probiotic or synbiotic supplementation during gestation and lactation on immune response, intestinal morphology, and microbiota community of offspring piglets. The sows were assigned randomly to one of four groups, control group (basal diet), antibiotic group (basal diet supplemented with 50 g/t virginiamycin), probiotic group (basal diet supplemented with 200 mL/d probiotic fermentation broth per pig), or synbiotic group (basal diet supplemented with 200 mL/d probiotic fermentation broth per pig + 500 g/t xylo-oligosaccharides) during pregnancy and lactation periods. After weaning, two piglets close to the average body weight (BW) per litter were selected and fed a basal diet. Eight piglets with similar BW were selected from each group for sample collection at 65 d-old. The results showed that plasma interleukin (IL)-2 and lipopolysaccharide concentrations were decreased (P < 0.05) in the probiotic group, while the immunoglobulin A (IgA) concentration in the probiotic and synbiotic groups was increased (P < 0.05), when compared with the control group. The jejunal IL-10, interferon-α, and secretory IgA (sIgA) concentrations were increased (P < 0.05) in the probiotic and synbiotic groups, as well as the ileal sIgA concentration in the probiotic group. The jejunal villus height (VH) and the ratio of VH to crypt depth were increased (P < 0.05) in the probiotic group, as well as the ileal VH in the synbiotic group. Furthermore, the piglets from the antibiotic group exhibited a lower microbiota diversity in the jejunum and ileum. The piglets from the synbiotic group had higher relative abundances of Actinobacteria, Bifidobacterium, Turicibacter, and Clostridium in the jejunum compared with the antibiotic group. Dietary probiotic treatment increased (P < 0.05) the relative abundance of Psychrobacter in the ileum compared with the antibiotic and control groups. Spearman's correlation analysis revealed that the relative abundances of Bifidobacterium, Clostridium, and Blautia in the jejunum and Psychrobacter in the ileum, were positively correlated with the alterations of immunoglobulin and cytokines. Collectively, these findings suggest that maternal interventions with probiotic or synbiotic are promising strategies for improving the immune response of offspring piglets by altering the gut microbiota.

Keywords: Bama mini-pigs, immune function, intestinal microbiota, probiotic, synbiotic

Introduction

The gut microbiota exerts important roles in gut function, host metabolism, immune development, and cell proliferation and differentiation during early life (1, 2). Early colonization of intestinal microbiota promotes the development and maturation of the intestinal immune system and barrier function of the host (3). Maternal diet during pregnancy and lactation periods is one of the pivotal factors affecting the growth and development of the offspring (4). During pregnancy and lactation, maternal body undergoes substantial hormonal, immunological, and metabolic changes that affect their gut microbiota (5). Although still controversial, more and more evidence suggests that the mother's intestine microbes could colonize the fetus in utero (6–8). Therefore, maternal microbiota could be transmitted to the offspring through direct contact during parturition or breastfeeding during lactation (9, 10). In humans, it has also been proposed that the administration of probiotics during the perinatal and lactation periods favors beneficial bacteria colonization in the infant's gut (11, 12). Recent studies also showed that maternal commensal microbiota can induce antibodies that recognize antigens expressed by pathogenic bacteria and protect offspring from infection (13). In this context, increasing the maternal beneficial microbiota through dietary supplementation during gestation and lactation periods has been considered a window of opportunity to modulate the intestinal health in offspring.

A previous study has reported that supplementing Enterococcus faecium to sows' diets during late pregnancy and lactation periods improved the offspring's body weight and average daily gain, and altered the fecal microbiota (14). Supplementing Bacillus subtilis to sows' diets during gestation and lactation periods reduced pathogenic bacteria and established beneficial bacteria (such as Lactobacillus) in neonatal piglets (15). Our previous studies showed that dietary probiotics supplementation to sows improved the birth weight of suckling piglets (16). Moreover, dietary synbiotics supplementation improved the piglet survival rate, but did not affect the litter size, born alive, and average body weight (17). In addition, maternal synbiotic supplementation increased the average daily gain of 65 d-old piglets; and maternal probiotic or synbiotic supplementation reduced the feed/gain ratio of 65 d-old piglets (unpublished data). However, the effects of supplementing probiotic or synbiotic to sows' diets on the immune system and gut microbiota composition of weaned piglets are poorly understood. Therefore, the present study aimed to determine the effect of maternal probiotic or synbiotic supplementation on the gut microbiota and immune response in offspring weaned piglets.

Materials and Methods

Animals, Treatments, and Diets

A total of 64 pregnant Bama mini-pigs during 3–5 parities with similar initial body weight (about 90 kg) were randomly assigned to one of four groups, with 16 sows per group. The four groups were as follows: control group (basal diet), antibiotic group (basal diet supplemented with 50 g/t virginiamycin), probiotic group (basal diet supplemented with probiotic fermentation broth 200 mL/d per pig), and synbiotic group [basal diet supplemented with probiotic fermentation broth 200 mL/d per pig + 500 g/t xylo-oligosaccharides (XOS)]. The compound probiotic fermentation broth was purchased from Hunan LiFeng Biotechnology Co., Ltd. (Changsha, China) and contained ≥1.2 × 108 CFU/g viable bacteria (Lactobacillus Plantarum B90 CGMCC1.12934 ≥1.0 × 108 CFU/g and Saccharomyces cerevisiae P11 CGMCC2.3854 ≥0.2 × 108 CFU/g). The viable microbe number in the broth was counted by the plate counting method. Then the fermentation broth was mixed with the diet according to the dose mentioned above per day before feeding. The XOS was purchased from Shandong Longlive Biotechnology Co., Ltd. (Shandong, China) and composed of xylobiose, xylotriose, and xylotetraose (accounting for ≥35%), which met the Chinese feed additive recommended requirements of XOS (GB/T23747-2009). The dose of compound probiotic and XOS is referred to the previous studies (17, 18).

After insemination, the sows were individually housed in gestation crates (2.2 m × 0.6 m) from day 0 (mating) to day 105 of pregnancy and then moved to the individual farrowing crates (2.2 m × 1.8 m) until weaning. The sows were fed 0.8, 1.0, 1.2, 1.5, and 2.0 kg of pregnant diets during 1–15, 16–30, 31–75, 76–90, and 91–105 days of pregnancy, respectively, fed 1.0 kg pregnant diets before a week of parturition, and ad libitum from delivery to weaning. The sows were allowed to drink freely throughout the trial (19).

The piglets were weaned at 28 ± 3 days and offered creep feed for 1 week. After 1 week of adaption, two piglets close to the average body weight (BW) per litter were transferred to the nursery facility and paired with two piglets from another sow within the same treatment. Four piglets were assigned to one pen, with eight pens (replicates) per group. The piglets were allowed ad libitum consumption of basal diets (provided twice daily; at 8:00 and 17:00). Each pen was equipped with a single-hole feeder and a water nipple to allow ad libitum access to water for sows and piglets. The composition and nutrients levels of basal diets for sows and piglets met the Chinese nutrient requirements of swine in China (NY/T65-2004), and the premixes met the NRC recommended requirements (20) (Supplementary Tables 1, 2).

Sample Collection

Eight piglets (one piglet per pen) were randomly chosen from each group, fasted for 12 h, and then weighed at 65 d-old. Blood samples were collected via the precaval vein of each pig and centrifuged at 3,500 × g for 10 min at 4°C to obtain the plasma and then stored at −20°C for future analyses. Following the blood sampling, all piglets were exsanguinated after electrical stunning (120 V, 200 HZ). The contents of the jejunum (10 cm below the flexure of duodenum-jejunum) and ileum (10 cm above the ileocecal junction) were collected and stored at −80°C for microbial composition and metabolites analyses. The jejunum and ileum segments (~2 cm in length) were washed with phosphate buffered saline (PBS) to remove intestinal contents and then fixed with 4% paraformaldehyde for analyzing intestinal morphology. The jejunum and ileum tissues were excised and washed with PBS. Then the mucosa samples were collected and immediately stored at −80°C for cytokines and secretory immunoglobulin A (sIgA) analyses.

Analysis of Plasma Cytokines, Immunoglobulins, Endotoxin, and D-Lactic Acid

The plasma concentrations of interleukin-2 (IL-2), IL-6, IL-10, tumor necrosis factor-alpha (TNF-α), interferon-alpha (IFN-α), interferon-gamma (IFN-γ), IgA, IgM, lipopolysaccharide (LPS), and D-lactic acid (D-LA) were determined using ELISA assay kits (Mei mian, Jiangsu, China) according to the manufacturer's protocol.

Analysis of Intestinal Cytokines and sIgA Levels

The jejunal and ileal mucosa samples about 0.1000 g were homogenized with ice-cold physiological saline (1:9, w/v) and centrifuged at 2,000 × g for 20 min at 4°C, and then the supernatants were separated for determining cytokines and sIgA levels. The levels of IL-2, IL-6, IL-10, TNF-α, IFN-α, IFN-γ, and sIgA in the intestinal mucosa were measured using ELISA assay kits (Mei mian, Jiangsu, China) according to the manufacturer's protocol. The total protein levels of the supernatants were quantified using the Pierce BCA Protein Assay Kit (Thermo Scientific, Shanghai, China). The intestinal cytokines and sIgA levels were normalized to the total protein concentration (mg/L) of the supernatants.

Intestinal Histomorphology Analysis

The jejunum and ileum segments fixed with 4% paraformaldehyde solution were dehydrated and then embedded in paraffin. The tissues were cut into ~5-μm thick sections. Hematoxylin and eosin (H&E) staining was performed according to the previously described protocol (21). The digital images of intestinal morphology at 40 and 100 × magnification were captured using a light microscope (Olympus Bx51, Japan). Fifteen representative measures per tissue were used to measure the villus height (VH) and crypt depth (CD) using Image-Pro Plus software (version 6.0) in a blinded manner. The VH was defined as the distance from the crypt-villus junction to the tip of the villus, and the CD was defined as the distance from the bottom of the crypt to the crypt-villus junction, as described previously (22).

Microbial Metabolite Analysis

The short-chain fatty acids (SCFAs), including acetate, propionate, butyrate, isobutyrate, valerate, and isovalerate in the jejunum and ileum contents were determined by gas chromatography (Agilent Technologies 1206, Santa Clara, CA), as reported previously (23).

Intestinal Microbiota Analysis

Total microbial genomic DNA was extracted from the jejunal and ileal contents (~0.3000 g) using Mag-Bind® Stool DNA Kit (Omega, Guangzhou, China) following the manufacturer's instructions and stored at −20°C for further analysis. The concentration and quality of the extracted DNA were confirmed using a NanoDrop OneC Microvolume UV-Vis Spectrophotometer (Thermo Scientific, Waltham, USA) and 1.2% agarose gel electrophoresis. The V3–V4 region of the 16S rRNA genes were amplified with primers: 338F (5′-ACTCCTACGGGAGGCAGCA-3′) and 806R (5′-GGACTACHVGGGTWTCTAAT-3′). The PCR amplicons were purified with Vazyme VAHTSTM DNA Clean Beads and quantified using the Quant-iT PicoGreen dsDNA assay kit (Invitrogen, Carlsbad, USA). Purified amplicons were sequenced on an Illumina MiSeq platform (Illumina, San Diego, USA) with the MiSeq Reagent Kit v3 (600 cycles) according to the standard protocol by Shanghai Personal Biotechnology Co. Ltd. (Shanghai, China).

The QIIME2 pipeline was used to process the sequencing data as previously described (24). Briefly, raw sequencing reads exactly matched with the barcodes were assigned to each sample and identified as valid sequences. Low quality sequences were filtered by the following criteria (25): sequences lengths shorter than 150 bp, an average Phred score lower than 20, and ambiguous bases or mononucleotide repeats exceeding 8 bp. Paired-end reading was calculated using FLASH (v1.2.11) assembly (26). After chimera detection, the remaining high-quality sequences were clustered into operational taxonomic unit (OTU) with 97% sequence identity using USEARCH (v7.0.1090) (27). A representative sequence was selected from each OTU using default parameters. The OTU taxonomic classification was conducted by Ribosomal Database Project (RDP) Classifier trained on Greengene (V201305) reference database (28). All the raw Illumina pair-end read data involved in the present study were deposited in the NCBI Sequence read archive (SRA) database under accession number PRJNA718786.

Statistical Analyses

The plasma and intestinal immune parameters were analyzed by one-way ANOVA and the comparative analysis was conducted using the Tukey post-hoc test (SPSS 22.0; SPSS Inc., Chicago, IL, USA). The microbiota alpha diversity and abundance were analyzed by the Kruskal-Wallis rank-sum test. All data are presented as means ± SEM. The significance value and a trend toward difference were set at levels of P < 0.05 and 0.05 ≤ P < 0.10, respectively. Alpha diversity (including Chao1, Shannon, Simpson, and Observed_species) was assessed using the OTU table in QIIME2 software. Partial least squares discriminant analysis (PLS-DA) based on unweighted UniFrac distance with constrained ordination and supervised learning was performed to reveal the intestinal microbiota variation among samples. The relative abundances of jejunal and ileal microbiota at phylum and genus levels were analyzed by Meta stats (http://metastats.cbcb.umd.edu/). Linear discriminant analysis (LDA) effect size (LEfSe) analysis was used to compare differences at the genus level among the four groups. The Spearman correlations between immune-related indexes and intestinal microbiota were measured using the R package ggplot2 3.3.1 (https://www.r-project.org/).

Results

The Concentrations of Plasma Cytokines and Immunoglobulins in Offspring Piglets

As shown in Figure 1, the plasma concentrations of TNF-α and IgM in the probiotic group were higher (P < 0.05) than in the antibiotic group. The IgA concentration in the antibiotic, probiotic, and synbiotic groups was increased (P < 0.05) compared with the control group.

Figure 1.

Figure 1

Open in a new tab

Effects of maternal probiotic or synbiotic supplementation on the plasma cytokines concentrations of offspring piglets. Data are represented as means ± SEM, n = 8 per group. Different letters indicate significant differences among the groups (P < 0.05). IL, Interleukin; TNF-α, Tumor necrosis factor-alpha; IFN, Interferon; IgA, immunoglobulin A; IgM, immunoglobulin M; C, control group; A, antibiotic group; P, probiotic group; and S, synbiotic group.

The Concentrations of Cytokines and sIgA in the Jejunum and Ileum of Offspring Piglets

In the jejunal mucosa, the concentrations of IL-10, IFN-α, and sIgA were increased (P < 0.05) in the probiotic and synbiotic groups, as well as IFN-γ in the synbiotic group, when compared with the control group (Figure 2A). The sIgA concentration in the synbiotic group was higher (P < 0.05) than in the antibiotic group. However, no significant differences were observed in the concentrations of IL-2, IL-6, and TNF-α among the four groups. In the ileal mucosa, probiotic treatment increased (P < 0.05) the sIgA concentration compared with the control and antibiotic groups (Figure 2B).

Figure 2.

Figure 2

Open in a new tab

Effects of maternal probiotic or synbiotic supplementation on the concentrations of cytokines and sIgA in the (A) jejunum and (B) ileum of offspring piglets. Data are represented as means ± SEM, n = 8 per group. Different letters indicate significant differences among the groups (P < 0.05). IL, Interleukin; TNF-α, Tumor necrosis factor-alpha; IFN, Interferon; sIgA, secretory immunoglobulin A; C, control group; A, antibiotic group; P, probiotic group; and S, synbiotic group.

The Morphology and Permeability in the Jejunum and Ileum of Offspring Piglets

Compared with the control group, the VH in the jejunum was higher (P < 0.05) in the antibiotic, probiotic, and synbiotic groups (Figures 3A,B), while the ratio of VH to CD was higher (P < 0.05) in the probiotic group (Figures 3A,D). The VH in the ileum was higher (P < 0.05) in the antibiotic and synbiotic groups compared with the control group. However, no significant difference were observed in the CD of jejunum and ileum (Figure 3C). In addition, the plasma LPS level in the probiotic group was decreased (P < 0.05) compared with the control group (Figure 4).

Figure 3.

Figure 3

Open in a new tab

Effects of maternal probiotic or synbiotic supplementation on the intestinal morphology of offspring piglets. Histomorphology of the jejunum and ileum was observed by light microscopy after H&E staining. (A) The images of the jejunum and ileum morphology at 40 × and 100 × magnification were shown, respectively. (B) Statistical analysis of villus height (VH), (C) crypt depth (CD), and (D) the ratio of VH to CD. Data are represented as means ± SEM, n = 8 per group. Different letters indicate significant differences among the groups (P < 0.05). C, control group; A, antibiotic group; P, probiotic group; and S, synbiotic group.

Figure 4.

Figure 4

Open in a new tab

Effects of maternal probiotic and synbiotic supplementation on the plasma concentrations of D-lactate (D-LA) and Lipopolysaccharide (LPS) of offspring piglets. Data are represented as means ± SEM, n = 8 per group. Different letters indicate significant differences among the groups (P < 0.05). C, control group; A, antibiotic group; P, probiotic group; and S, synbiotic group.

The SCFAs Concentrations in the Jejunum and Ileum of Offspring Piglets

The ileal acetate concentration was higher by 50.8% in the synbiotic group than in the control group, but there was no statistically significant difference (Supplementary Table 3). In addition, the concentrations of propionate, valerate, isobutyrate, and isovalerate in several samples were below the detection level.

The Microbiota Diversity in the Jejunum and Ileum of Offspring Piglets

Based on the high-throughput sequencing, a total of 9,791,833 raw reads were generated from 32 jejunum samples and 32 ileum samples of offspring piglets. After removing the low-quality sequences, 7,648,982 effective tags were obtained and clustered into OTUs. Based on 97% sequence similarity, the V3–V4 region sequence was annotated as 9,302 bacterial OTUs in the jejunum, among which there were 541 shared bacterial OTUs; while the V3–V4 region sequence was annotated as 9,488 bacterial OTUs in the ileum, among which there were 469 shared bacterial OTUs (Figures 5A,B).

Figure 5.

Figure 5

Open in a new tab

Effects of maternal probiotic and synbiotic supplementation on microbial alpha diversity in the jejunum and ileum of offspring piglets. Venn diagrams for microbiota OTUs compositions in the (A) jejunum and (B) ileum. The microbiota diversity estimated by (C–F) Chao1, Shannon, Simpson, and Observed_species in the jejunum and (G–J) ileum, respectively. Partial least squares discrimination analysis (PLS-DA) of (K) jejunal and (L) ileal microbiota community of offspring piglets. Data are represented as means ± SEM, n = 8 per group. *P < 0.05. C, control group; A, antibiotic group; P, probiotic group; and S, synbiotic group.

The piglets from the antibiotic group exhibited a lower alpha diversity in both jejunum and ileum as evidenced by the reduced jejunal indexes of Shannon and Simpson indexes, as well as ileal Chao1 and Observed_species indexes (Figures 5C–J). In the jejunum and ileum, PLS-DA showed that the samples in the control, probiotic, and synbiotic groups were separated and clustered into distinct groups (Figures 5K,L).

The Microbiota Composition in the Jejunum and Ileum of Offspring Piglets

In the jejunum, Proteobacteria, Firmicutes, Actinobacteria, and Bacteroidetes were the predominant phyla, which accounted for 99.3% of the total bacteria (Figure 6A). The relative abundance of Actinobacteria in the synbiotic group was higher (P < 0.01) than that in the antibiotic group (Figure 6C), while the relative abundances of Bacteroidetes (P < 0.05) and [Thermi] (P = 0.080) were lower in the antibiotic group and as well as the relative abundance of [Thermi] (P = 0.086) in the probiotic group (Figures 6D,E) when compared with the control group. In the ileum, Firmicutes, Proteobacteria, Actinobacteria, and Bacteroidetes were the predominant phyla, which accounted for 99.7% of the total bacteria (Figure 7A). However, there was no significant difference at the phylum level among the four groups.

Figure 6.

Figure 6

Open in a new tab

Gut microbiota community composition in the jejunum of offspring piglets. Abundances of the jejunal microbiota at (A) phylum and (B) genus levels of offspring piglets. All phyla and the top 20 genera were listed. Comparison of relative abundances at (C–E) phylum and (F–I) genus levels were analyzed by the Kruskal-Wallis rank-sum test. *P < 0.05; **P < 0.01. C, control group; A, antibiotic group; P, probiotic group; and S, synbiotic group.

Figure 7.

Figure 7

Open in a new tab

Gut microbiota community composition in the ileum of offspring piglets. Abundances of the ileal microbiota at (A) phylum and (B) genus levels of offspring piglets. All phyla and the top 20 genera were listed. Comparison of relative abundances at (C–F) genus level was analyzed by the Kruskal-Wallis rank-sum test. *P < 0.05. C, control group; A, antibiotic group; P, probiotic group; and S, synbiotic group.

The 20 most dominant microbial genera in the jejunum and ileum are shown in Figures 6B, 7B. In the jejunum, the relative abundances of Bifidobacterium, Rothia, and Turicibacter were higher (P < 0.05) in the synbiotic group, as well as Clostridium (P = 0.068), when compared with the antibiotic group (Figures 6F–I). In the ileum, dietary probiotic supplementation increased (P < 0.05) the relative abundance of Psychrobacter compared with the antibiotic and control groups (Figure 7E). In addition, dietary synbiotic supplementation increased (P < 0.05) the relative abundance of Corynebacterium compared with the antibiotic group (Figure 7C). However, the antibiotic supplementation decreased (P < 0.05) the relative abundances of Gemella and SMB53 compared with the control group (Figures 7D,F).

To further explore the differences of intestinal microbiota communities among the four groups, the LEfSe analysis was performed at the genus level and presented the LDA score above 2.0. In the jejunum, a significant enrichment of Turicibacter, SMB53, Clostridium, Paracoccus, Thalassobius, Vibrio, Psychrobacter, and Blautia was observed in the synbiotic group, and Mogibacterium was the most abundant genera in the probiotic group (Figure 8A). In the ileum, Corynebacterium and Agrobacterium were enriched in the synbiotic group, while Dialister, Oleomonas, and Facklamia were enriched in the probiotic group (Figure 8B).

Figure 8.

Figure 8

Open in a new tab

The differentially abundant taxa among the four groups by LEfSe (LDA Effect Size) analysis. Histograms of a linear discriminant analysis (LDA) score (threshold: ≥ 2) in (A) jejunum and (B) ileum. n = 8 per group. C, control group; A, antibiotic group; P, probiotic group; and S, synbiotic group.

The Correlation of Intestinal Microbiota, Plasma Parameters, and Intestinal Immune-Related Indexes

As shown in Figure 9A, the relative abundance of jejunal Bifidobacterium showed a positive (P < 0.05) correlation with the plasma concentrations of IL-10 and TNF-α. The relative abundance of jejunal Rothia was positively (P < 0.05) correlated with the plasma concentrations of IL-2, IL-6, and IL-10. Meanwhile, the relative abundance of jejunal SMB53 was positively (P < 0.05) correlated with the plasma IL-6 concentration, and the relative abundance of jejunal Blautia was positively (P < 0.05) correlated with the plasma concentrations of IL-2 and IL-6. Moreover, the relative abundances of jejunal Turicibacter and Clostridium were positively (P < 0.05) correlated with the plasma IL-6 concentration. As shown in Figure 9B, the relative abundance of ileal Psychrobacter was positively (P < 0.05) correlated with the plasma concentrations of IL-2, IL-10, TNF-α, and IgM.

Figure 9.

Figure 9

Open in a new tab

The Spearman correlation between the (A) plasma immune-related parameters and jejunal microbiota; (B) plasma immune-related parameters and ileal microbiota; (C) jejunal immune-related parameters and jejunal microbiota; (D) ileal immune-related parameters and ileal microbiota. *P < 0.05. Cells are colored based upon the Spearman correlation coefficient between the significantly altered genera and immune-related parameters; the red and blue represents a significantly positive correlation and negative correlation, respectively.

As shown in Figure 9C, the relative abundance of jejunal Rothia was positively (P < 0.05) correlated with the jejunal sIgA concentration. The relative abundance of jejunal Bifidobacterium was negatively (P < 0.05) correlated with the jejunal IL-6 concentration. The relative abundance of jejunal Paracoccus was negatively (P < 0.05) correlated with the jejunal IL-2 concentration. As shown in Figure 9D, the relative abundance of ileal Psychrobacter was positively (P < 0.05) correlated with the ileal sIgA concentration.

Discussion

The gut microbiota of humans or animals is vital for immune system development, metabolism, and mucosal barrier function during early life (1, 2). In human studies, the modulation of microbiota composition by using probiotic or synbiotic during perinatal and early postnatal periods facilitates the colonization of potentially beneficial bacteria in the neonatal gut, which has been considered as a potential dietary strategy to reduce the risk of neonatal disease (29). However, the effects of maternal probiotic or synbiotic supplementation on intestinal health, especially on the immune function of offspring piglets are poorly understood. The present study showed that maternal probiotic or synbiotic supplementation improved intestinal epithelial morphology and enhanced systemic and intestinal immunity to some extent in the subsequent offspring, which is concomitant with alterations of intestinal microbiota composition.

The IgA is a major plasma immunoglobulin that protects the host against microbes. Several studies have reported that Bifidobacterium bifidum and Bacillus subtilis could increase the levels of immunoglobulins in the host's blood (30, 31). In the present study, maternal dietary probiotic or synbiotic supplementation increased the plasma IgA concentration of offspring piglets, suggesting that these animals gained an enhanced humoral immunity. Thus, our findings further demonstrated the beneficial effect of maternal probiotic or synbiotic supplementation on the systemic immune of offspring piglets.

Intestinal mucosal barrier function is vital to maintain intestinal homeostasis and morphology (32). Increasing studies have demonstrated that several probiotics facilitated the intestinal epithelial barrier function in mammals (30, 33, 34). In the present study, dietary probiotic or synbiotic supplementation to sows improved the intestinal physical barrier function, as evidenced by the increased VH and VH/CD ratio in the jejunum of offspring piglets. Moreover, the reduced intestinal epithelial permeability indicating a favorable mucosa structure for nutrient absorption and digestion (35). These alterations might result in the increased growth performance of offspring piglets.

The immunological barrier function is one of the vital functions for intestinal homeostasis (36). Previous studies have reported that probiotics could induce the macrophages and dendritic cells to secrete immune cytokines to trigger the intestinal immune system (37). Lactobacillus frumenti and Bifidobacterium bifidum were found to facilitate intestinal sIgA secretion (30, 34). Moreover, Lactobacillus fermentum supplementation in rats during pregnancy and lactation periods increased the intestinal IgA concentration in those pups (38). In the present study, maternal probiotic or synbiotic supplementation increased jejunal IFN-α concentration, as well as the jejunal and ileal sIgA concentration in the offspring piglets, which were consistent with previous studies. Recently, Psychrobacter bacteria have been recognized as a potential probiotic, which could improve the growth performance and upregulate the immune-related genes (39, 40). In the present study, the increased ileal sIgA might be resulted from the increased abundance of ileal Psychrobacter, which were positively correlated with the ileal sIgA. These findings suggested that maternal probiotic or synbiotic supplementation could enhance the intestinal mucosal immunity.

The gut microbial diversity plays an important role in maintaining a stable microbial community (41). In the present study, maternal probiotic or synbiotic supplementation had no effect on the intestine microbial richness and diversity. A recent study also reported that maternal administration of Lactobacillus fermentum CECT5716 failed to modify the cecal alpha diversity in offspring rats (38). However, maternal antibiotic supplementation dramatically decreased the microbial alpha diversity in both jejunum and ileum, which is consistent with a previous report that dietary antibiotic supplementation induced microbial dysbiosis by reducing the abundance and diversity of commensal microbes (42). Accordingly, the beta-diversity analysis showed that maternal probiotic or synbiotic supplementation significantly altered the microbial community in the small intestine of offspring piglets.

In the present study, maternal synbiotic supplementation increased the relative abundances of Actinobacteria, Bifidobacterium, Turicibacter, and Clostridium in the jejunum of offspring piglets. Several studies have reported that Turicibacter induces intestinal T-cell activation in the rat hypertension model (43). Clostridium (including Clostridium cluster IV and XIVa), as a potential probiotic, exerts lots of benefits on intestinal homeostasis (44). Actinobacteria (i.e., Bifidobacterium) is the key players in maintaining gut barrier homeostasis (30, 45). A previous study also reported that Bifidobacterium species can produce acetate and lactate during carbohydrate fermentation (46). The increased abundance of Bifidobacterium maybe contributes to the numerically increased ileal acetate concentration in the present study. Acetate, as a major SCFAs, was regarded as the mediator in the crosstalk between the intestinal microbiota and immune regulation (47). These findings may explain the enhanced intestinal mucosal immunity after dietary supplementing synbiotic to sows in the present study. In addition, the jejunal Bifidobacterium abundance showed a positive correlation with the plasma TNF-α concentration, and jejunal Turicibacter and Clostridium abundances were positively correlated with the plasma IL-6 concentration. Therefore, the alteration of these gut microbiota by maternal probiotic or synbiotic supplementation may attribute to the changes of immune-related parameters in the offspring piglets. Further studies are needed to determine the possible causal relationship.

Conclusion

Maternal probiotic or synbiotic supplementation improved intestinal epithelial morphology and intestinal immunity, and these two additives exhibited similar effects. Alterations in the relative abundances of Bifidobacterium, Clostridium, Turicibacter, and Psychrobacter in the jejunum and ileum may be associated with intestinal immunity. These findings provide new insight that maternal interventions with probiotic or synbiotic are promising strategies for improving the immune response of offspring piglets by altering the gut microbiota.

Data Availability Statement

The datasets presented in this study can be found in online repositories. The names of the repository/repositories and accession number(s) can be found at: https://www.ncbi.nlm.nih.gov/sra/?term=PRJNA718786.

Ethics Statement

The animal study was reviewed and approved by Animal Care and Use Committee of the Institute of Subtropical Agriculture, Chinese Academy of Sciences.

Author Contributions

XK and KW designed the experiment and wrote the manuscript. CH, WT, MA, QZ, and QH carried out the animal experiment, sample collection, and sample analysis. KW performed the statistical analyses. All authors read and approved the final manuscript.

Conflict of Interest

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.

Acknowledgments

We thank staff members and postgraduate students from Hunan Provincial Key Laboratory of Animal Nutritional Physiology and Metabolic Process for collecting samples and technicians from the CAS Key Laboratory of Agro-ecological Processes in Subtropical Region for providing technical assistance.

Footnotes

Funding. The present study was jointly supported by the National Key Research and Development Project (2018YFD0500404-4), National Natural Science Foundation of China (31772613), Special Funds for Construction of Innovative Provinces in Hunan Province (2019RS3022), and Open Research Foundation from Hunan Provincial Key Laboratory of Animal Nutritional Physiology and Metabolic Process (ISA2020111).

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fnut.2021.686053/full#supplementary-material

Click here for additional data file. (177.1KB, pdf)

References

  • 1.Tanaka M, Nakayama J. Development of the gut microbiota in infancy and its impact on health in later life. Allergol Int. (2017) 66:515–22. 10.1016/j.alit.2017.07.010 [DOI] [PubMed] [Google Scholar]
  • 2.Collado MC, Cernada M, Bauerl C, Vento M, Perez-Martinez G. Microbial ecology and host-microbiota interactions during early life stages. Gut Microbes. (2012) 3:352–65. 10.4161/gmic.21215 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 3.Kabat AM, Srinivasan N, Maloy KJ. Modulation of immune development and function by intestinal microbiota. Trends Immunol. (2014) 35:507–17. 10.1016/j.it.2014.07.010 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 4.Kominiarek MA, Rajan P. Nutrition recommendations in pregnancy and lactation. Med Clin North Am. (2016) 100:1199–215. 10.1016/j.mcna.2016.06.004 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 5.Koren O, Goodrich JK, Cullender TC, Spor A, Laitinen K, Backhed HK, et al. Host remodeling of the gut microbiome and metabolic changes during pregnancy. Cell. (2012) 150:470–80. 10.1016/j.cell.2012.07.008 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 6.Rackaityte E, Halkias J, Fukui EM, Mendoza VF, Hayzelden C, Crawford ED, et al. Viable bacterial colonization is highly limited in the human intestine in utero. Nat Med. (2020) 26:599–607. 10.1038/s41591-020-0761-3 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 7.Willyard C. Could baby's first bacteria take root before birth? Nature. (2018) 553:264–66. 10.1038/d41586-018-00664-8 [DOI] [PubMed] [Google Scholar]
  • 8.Collado MC, Rautava S, Aakko J, Isolauri E, Salminen S. Human gut colonisation may be initiated in utero by distinct microbial communities in the placenta and amniotic fluid. Sci Rep. (2016) 6:23129. 10.1038/srep23129 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 9.Wampach L, Heintz-Buschart A, Fritz JV, Ramiro-Garcia J, Habier J, Herold M, et al. Birth mode is associated with earliest strain-conferred gut microbiome functions and immunostimulatory potential. Nat Commun. (2018) 9:5091. 10.1038/s41467-018-07631-x [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 10.Pannaraj PS, Li F, Cerini C, Bender JM, Yang S, Rollie A, et al. Association between breast milk bacterial communities and establishment and development of the infant gut microbiome. JAMA Pediatr. (2017) 171:647–54. 10.1001/jamapediatrics.2017.0378 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 11.Schultz M, Göttl C, Young RJ, Iwen P, Vanderhoof JA. Administration of oral probiotic bacteria to pregnant women causes temporary infantile colonization. J Pediatr Gastroenterol Nutr. (2004) 38:293–7. 10.1097/00005176-200403000-00012 [DOI] [PubMed] [Google Scholar]
  • 12.Martín R, Jiménez E, Heilig H, Fernández L, Marín ML, Zoetendal EG, et al. Isolation of Bifidobacteria from breast milk and assessment of the bifidobacterial population by PCR-denaturing gradient gel electrophoresis and quantitative real-time PCR. Appl Environ Microbiol. (2009) 75:965–9. 10.1128/AEM.02063-08 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 13.Zheng W, Zhao W, Wu M, Song X, Caro F, Sun X, et al. Microbiota-targeted maternal antibodies protect neonates from enteric infection. Nature. (2020) 577:543–8. 10.1038/s41586-019-1898-4 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 14.Lan R, Kim I. Enterococcus faecium supplementation in sows during gestation and lactation improves the performance of sucking piglets. Vet Med Sci. (2020) 6:92–9. 10.1002/vms3.215 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 15.Baker AA, Davis E, Spencer JD, Moser R, Rehberger T. The effect of a Bacillus-based direct-fed microbial supplemented to sows on the gastrointestinal microbiota of their neonatal piglets. J Anim Sci. (2013) 91:3390–9. 10.2527/jas.2012-5821 [DOI] [PubMed] [Google Scholar]
  • 16.Ma C, Gao QK, Zhang WH, Zhu Q, Kong XF. Effects of dietary Lactobacillus and Yeast fermentation broth on reproductive performance, colostrum composition and plasma biochemical indexes of sows. Chin J Anim Nutr. (2020) 32:129–37. 10.3969/j.issn.1006-267x.2020.01.018 [DOI] [Google Scholar]
  • 17.Ma C, Zhang WH, Gao QK, Zhu Q, Song MT, Ding H, et al. Dietary synbiotic alters plasma biochemical parameters and fecal microbiota and metabolites in sows. J Funct Foods. (2020) 75:104221. 10.1016/j.jff.2020.104221 [DOI] [Google Scholar]
  • 18.Tan B, Ji YJ, Ding H, Li FW, Zhou QH, Kong XF. Effects of xylo-oligosaccharide on growth performance, diarrhea rate and plasma biochemical parameters of weaned piglets. Chin J Anim Nutr. (2016) 28:2556–63. 10.3969/j.issn.1006-267x.2016.08.028 [DOI] [Google Scholar]
  • 19.Ma C, Gao QK, Zhang WH, Azad MAK, Kong XF. Alterations in the blood parameters and fecal microbiota and metabolites during pregnant and lactating stages in Bama mini pigs as a model. Mediators Inflamm. (2020) 2020:8829072. 10.1155/2020/8829072 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 20.National Research Council (NRC) . Nutrient Requirements of Swine. 11th revised ed. Washington, DC: The National Academies Press; (2012). [Google Scholar]
  • 21.Hu J, Nie YF, Chen S, Xie C, Fan Q, Wang Z, et al. Leucine reduces reactive oxygen species levels via an energy metabolism switch by activation of the mTOR-HIF-1alpha pathway in porcine intestinal epithelial cells. Int J Biochem Cell Biol. (2017) 89:42–56. 10.1016/j.biocel.2017.05.026 [DOI] [PubMed] [Google Scholar]
  • 22.Igarashi M, Guarente L. mTORC1 and SIRT1 cooperate to foster expansion of gut adult stem cells during calorie restriction. Cell. (2016) 166:436–50. 10.1016/j.cell.2016.05.044 [DOI] [PubMed] [Google Scholar]
  • 23.Kong XF, Ji YJ, Li HW, Zhu Q, Blachier F, Geng MM, et al. Colonic luminal microbiota and bacterial metabolite composition in pregnant Huanjiang mini-pigs: effects of food composition at different times of pregnancy. Sci Rep. (2016) 6:37224. 10.1038/srep37224 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 24.Caporaso JG, Kuczynski J, Stombaugh J, Bittinger K, Bushman FD, Costello EK, et al. QIIME allows analysis of high-throughput community sequencing data. Nat Methods. (2010) 7:335–6. 10.1038/nmeth.f.303 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 25.Chen H, Jiang W. Application of high-throughput sequencing in understanding human oral microbiome related with health and disease, Front Microbiol. (2014) 5:508. 10.3389/fmicb.2014.00508 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 26.Magoc T, Salzberg SL. FLASH: fast length adjustment of short reads to improve genome assemblies. Bioinformatics. (2011) 27:2957–63. 10.1093/bioinformatics/btr507 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 27.Edgar RC. UPARSE: highly accurate OTU sequences from microbial amplicon reads. Nat Methods. (2013) 10:996–8. 10.1038/nmeth.2604 [DOI] [PubMed] [Google Scholar]
  • 28.DeSantis TZ, Hugenholtz P, Larsen N, Rojas M, Brodie EL, Keller K, et al. Greengenes, a chimera-checked 16S rRNA gene database and workbench compatible with ARB. Appl Environ Microbiol. (2006) 72:5069–72. 10.1128/AEM.03006-05 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 29.Sanz Y. Gut microbiota and probiotic in maternal and infant health. Am J Clin Nutr. (2011) 94:2000S−5S. 10.3945/ajcn.110.001172 [DOI] [PubMed] [Google Scholar]
  • 30.Tanaka K, Tsukahara T, Yanagi T, Nakahara S, Furukawa O, Tsutsui H, et al. Bifidobacterium bifidum OLB6378 simultaneously enhances systemic and mucosal humoral immunity in low birth weight infants: a non-randomized study. Nutrients. (2017) 9:195. 10.3390/nu9030195 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 31.Guo M, Wu F, Hao G, Qi Q, Li R, Li N, et al. Bacillus subtilis improves immunity and disease resistance in rabbits. Front Immunol. (2017) 8:354. 10.3389/fimmu.2017.00354 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 32.Odenwald MA, Turner JR. The intestinal epithelial barrier: a therapeutic target? Nat Rev Gastroenterol Hepatol. (2016) 14:9–21. 10.1038/nrgastro.2016.169 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 33.Wan LY, Chen ZJ, Shah NP, El-Nezami H. Modulation of intestinal epithelial defense responses by probiotic bacteria. Crit Rev Food Sci Nutr. (2016) 56:2628–41. 10.1080/10408398.2014.905450 [DOI] [PubMed] [Google Scholar]
  • 34.Hu J, Chen L, Zheng W, Shi M, Liu L, Xie C, et al. Lactobacillus frumenti facilitates intestinal epithelial barrier function maintenance in early-weaned piglets. Front Microbiol. (2018) 9:897. 10.3389/fmicb.2018.00897 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 35.Yin J, Li F, Kong X, Wen C, Guo Q, Zhang L, et al. Dietary xylo-oligosaccharide improves intestinal functions in weaned piglets. Food Funct. (2019) 10:2701–9. 10.1039/C8FO02485E [DOI] [PubMed] [Google Scholar]
  • 36.Rescigno M. The intestinal epithelial barrier in the control of homeostasis and immunity. Trends Immunol. (2011) 32:256–64 10.1016/j.it.2011.04.003 [DOI] [PubMed] [Google Scholar]
  • 37.Galdeano CM, de Moreno de LeBlanc A, Vinderola G, Bonet ME, Perdigon G. Proposed model: mechanisms of immunomodulation induced by probiotic bacteria. Clin Vaccine Immunol. (2007) 14:485–92. 10.1128/CVI.00406-06 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 38.Azagra-Boronat I, Tres A, Massot-Cladera M, Franch A, Castell M, Guardiola F, et al. Lactobacillus fermentum CECT5716 supplementation in rats during pregnancy and lactation impacts maternal and offspring lipid profile, immune system and microbiota. Cells. (2020) 9:575. 10.3390/cells9030575 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 39.Yang HL, Sun YZ, Ma RL, Li JS, Huang KP. Probiotic Psychrobacter sp. improved the autochthonous microbial diversity along the gastrointestinal tract of grouper epinephelus coioides. J Aquac Res Dev. (2011) s1:001. 10.4172/2155-9546.S1-001 [DOI] [Google Scholar]
  • 40.Saad SO, Hamdan AM, El-Sayed AFM, Hafez EE. Evaluation of marine psychrophile, Psychrobacter namhaensis so89, as a probiotic in nile tilapia (oreochromis niloticus) diets. Fish Shellfish Immunol. (2017) 61:194–200. 10.1016/j.fsi.2017.01.001 [DOI] [PubMed] [Google Scholar]
  • 41.Li H, Qu J, Li T, Wirth S, Zhang Y, Zhao X, et al. Diet simplification selects for high gut microbial diversity and strong fermenting ability in high-altitude pikas. Appl Microbiol Biotechnol. (2018) 102:6739–51. 10.1007/s00253-018-9097-z [DOI] [PubMed] [Google Scholar]
  • 42.Looft T, Allen HK. Collateral effects of antibiotics on mammalian gut microbiomes. Gut Microbes. (2012) 3:463–7. 10.4161/gmic.21288 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 43.Toral M, Robles-Vera I, de la Visitacion N, Romero M, Sanchez M, Gomez-Guzman M, et al. Role of the immune system in vascular function and blood pressure control induced by faecal microbiota transplantation in rats. Acta Physiol. (2019) 227:e13285. 10.1111/apha.13285 [DOI] [PubMed] [Google Scholar]
  • 44.Guo P, Zhang K, Ma X, He P. Clostridium species as probiotic: potentials and challenges. J Anim Sci Biotechnol. (2020) 11:24. 10.1186/s40104-019-0402-1 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 45.Martins FS, Silva AA, Vieira AT, Barbosa FH, Arantes RM, Teixeira MM, et al. Comparative study of Bifidobacterium animalis, Escherichia coli, Lactobacillus casei and Saccharomyces boulardii probiotic properties. Arch Microbiol. (2009) 191:623–30. 10.1007/s00203-009-0491-x [DOI] [PubMed] [Google Scholar]
  • 46.Audrey R, Marija S, David L, Frédéric L, Luc DV. Bifidobacteria and butyrate-producing colon bacteria: importance and strategies for their stimulation in the human gut. Front Microbiol. (2016) 7:1030. 10.3389/fmicb.2016.00979 [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 47.Parada Venegas D, De la Fuente MK, Landskron G, González MJ, Quera R, Dijkstra G, et al. Short chain fatty acids (SCFAs)-mediated gut epithelial and immune regulation and its relevance for inflammatory bowel diseases. Front Immunol. (2019) 11:277. 10.3389/fimmu.2019.01486 [DOI] [PMC free article] [PubMed] [Google Scholar]

Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

Click here for additional data file. (177.1KB, pdf)

Data Availability Statement

The datasets presented in this study can be found in online repositories. The names of the repository/repositories and accession number(s) can be found at: https://www.ncbi.nlm.nih.gov/sra/?term=PRJNA718786.

Articles from Frontiers in Nutrition are provided here courtesy of Frontiers Media SA

RESOURCES