The Probiotic Combination of Bifidobacterium longum subsp. infantis CECT 7210 and Bifidobacterium animalis subsp. lactis BPL6 Reduces Pathogen Loads and Improves Gut Health of Weaned Piglets Orally Challenged with Salmonella Typhimurium.

Probiotics have been demonstrated to be useful to enhance gut health and prevent gastrointestinal infections in humans. Additionally, some multi-strain probiotic combinations have been suggested to have greater efficacy than single strains. The objective of this study is to demonstrate the potential of a combination of the probiotic strains: Bifidobacterium longum subsp. infantis CECT 7210 (brand name B. infantis IM1®) and B. animalis subsp. lactis BPL6 to enhance gut health and to ameliorate the outcome of a Salmonella challenge using a weaning piglet model. Seventy-two 28-day-old weanling piglets, 7.7 (±0.28) kg of body-weight, were distributed in a 2 × 2 factorial design; treated or not with the probiotic combination and challenged or not with the pathogen. Animals were orally challenged after an adaptation period (Day 8) with a single dose (5 × 108 cfu) of Salmonella Typhimurium. One animal per pen was euthanized on Day 12 (Day 4 post-inoculation [PI]) and Day 16 (Day 8 PI). All parameters responded to the challenge and 4 deaths were registered, indicating a severe but self-limiting challenge. Improvements registered in the challenged animals due to the probiotic were: increased voluntary feed-intake (P probiotic × challenge = 0.078), reduced fecal excretion of Salmonella (P = 0.028 at Day 1 PI and P < 0.10 at Days 3 and 5 PI), decreased rectal temperature (P probiotic × day = 0.048) and improvements in the villous:crypt ratio (P probiotic × challenge < 0.001). Moreover, general probiotic benefits were observed in both challenged and non-challenged groups: decreased diarrhea scores of the PI period (P = 0.014), improved fermentation profiles on Day 8 PI (increased ileal acetic acid [P = 0.008] and a tendency to lower colonic ammonia concentrations [P = 0.078]), stimulation of intestinal immune response by increasing villous intraepithelial lymphocytes (P = 0.015 on Day 8 PI) and an improved villous:crypt ratio (P = 0.011). In conclusion, the multi-strain probiotic had a positive effect on reducing pathogen loads and alleviating animals in a Salmonella challenge. In addition, enhanced gut health and immunity was recorded in all animals receiving the probiotic, indicating an improvement in the post-weaning outcome.

Introduction

Salmonella spp. enteric infections are among the most common diarrhea-associated causes of morbidity and mortality (CDC, 2013), especially in children up to 5 years of age (Lanata et al., 2013). In fact, newborn babies are considered to be especially vulnerable, as their immune system is still not fully developed and may be prone to infections by opportunistic pathogens (Lanata et al., 2013; Thanabalasuriar and Kubes, 2014). Altogether, Salmonella infections are estimated to be responsible for up to 155,000 deaths, when considering the global population (Majowicz et al., 2010), and over 100,000 human clinical cases are reported each year only in the EU, with an estimated overall economic burden of human salmonellosis of 3 billion euros a year (EFSA, 2013).

Probiotics and their metabolites have been suggested to play an important role in the formation or establishment of well-balanced, indigenous, intestinal microbiota in new-borne infants and adults (Gill, 2003; Salazar et al., 2009). Furthermore, the administration of probiotic microorganisms in milk formulas has well-documented benefits, including improvements in infections, diarrhea, allergic disorders, various gut pathogens and inflammatory diseases in children (Bin-Nun et al., 2005; Collado et al., 2007c; Minocha, 2009). For instance, remarkable beneficial effects against Salmonella have been documented by the Bifidobacterium spp. genus, with well-documented research in vitro (Liévin et al., 2000; Tanner et al., 2016) and in vivo using animal models (Shu et al., 2000; Silva et al., 2004; Zacarías et al., 2014). In particular, one of the strains conforming the probiotic combination tested in this study, Bifidobacterium longum subsp. infantis CECT 7210 (B. infantis IM1®), has demonstrated a reduction in ETEC K88 colonization and Salmonella fecal shedding in an in vivo model with weanling pigs (Barba-Vidal et al., 2017) and protective effects against a rotavirus infection in vitro and in a murine model (Moreno Muñoz et al., 2011).

Multi-strain and multi-species probiotic combinations have been suggested to have greater efficacy than single strains, as complementary or even synergistic effects can be achieved in the host when given together in comparison to giving them separately (Timmerman et al., 2004; Collado et al., 2007b; Chapman et al., 2011). Nevertheless, each specific probiotic combination should be tested, and further research efforts are needed. In this study, we hypothesize that combining the probiotic strain of B. longum subsp. infantis CECT 7210 with B. animalis subsp. lactis BPL6 could improve gut health. The objective of this work was, therefore, to demonstrate the potential of this probiotic combination to enhance gut health in human early-life stages and to ameliorate the outcome of a Salmonella challenge using a weaning piglet model.

Materials and Methods

The experiment was performed at the Experimental Unit of the Universitat Autònoma de Barcelona (UAB) and received prior approval (Permit No. CEAAH1619) from the Animal and Human Experimental Ethical Committee of this Institution. The treatment, management, housing, husbandry and slaughtering conditions conformed to European Union Guidelines (European Commission, 2010), and all efforts were made to minimize animal suffering.

Animals and Housing

The trial was conducted as a Level 2 High-Risk Biosecurity Procedure, with appropriate training of the personnel involved. A total of 72 male piglets (Large White × Landrace) from a high-sanitary-status farm and from mothers serologically negative to Salmonella were used. Animals were weaned at 28 (±3) days of age, 7.7 (±0.28) kg body-weight (BW) on average, and were transported to the UAB facilities, where they were placed in three rooms of eight pens each (24 pens, three animals per pen), taking initial BW into account for a similar average BW within pens. The pens were allocated to four treatment groups following an unbalanced 2 × 2 factorial arrangement (factors being probiotic and pathogen challenge), with eight replicates per treatment for the challenged animals and four replicates for the non-challenged group. The treatments were, therefore: (1) no challenge + no probiotic (NN); (2) no challenge + probiotic (NP); (3) challenged + no probiotic (CN) and (4) challenged + probiotic (CP). Two rooms were challenged with pathogens and one was left unchallenged. In each room, probiotic treatment was distributed among four pens on one side of the room, and the four control pens were on the other side of the room, separated by a corridor in between.

Pigs were maintained under a 14:30 h light/9:30 h dark lighting regimen. Each pen (2 m2) had a feeder and a water nipple to provide feed and water for ad libitum consumption. The weaning rooms were equipped with automatic heating, forced ventilation and an individual heat-light per pen. The experiment was conducted during the spring season (April), with an average room temperature of 26°C (±4°C). The experimental treatments were distributed evenly among the three rooms.

Experimental Products and Diets

The probiotic treatment was supplied by Ordesa S.L., and it consisted of a daily dosage (109 colony-forming units [cfu]) of a combination of B. longum subsp. infantis CECT 7210 (B. infantis IM1®) and B. animalis subsp. lactis BPL6 (B. lactis BPL6), supplemented in a 2 mL solution. The control group received, as a placebo, the same amount of carrier. During the experimental period, pigs received the treatment orally and individually, in a daily pattern using disposable 2 mL syringes without a needle. The probiotic tested was a single batch of lyophilized bacteria, which was re-suspended and administered every day, in less than 1 h time period. Viability of probiotic administered was verified by plating bacteria shortly after re-suspending the probiotic, and 1 and 2 h later stored at room temperature. Serial dilutions of the suspension were performed in Man Rogosa Sharpe (MRS) broth (Oxoid; Madrid, Spain) + 0.25% cysteine (Sigma–Aldrich; Madrid, Spain), plated in MRS-C agar (Oxoid; Madrid, Spain), incubated at 37°C in anaerobic conditions for 48 h and manually counted. Colony forming units were always maintained in a logarithm scale of 109 cfu/g.

A pre-starter diet without additives (Table ) was formulated to satisfy the nutrient requirement standards for pigs of this age (NRC, 2012) and was given in a mash form.

Bacterial Strain

The bacterial strain used in the present study was a Salmonella Typhimurium var. Monophasic (formula: 4,5,12:i:-, resistance profile: ACSSuT-Ge, Fagotype: U302) that was isolated from a salmonellosis outbreak (mainly enteric and with sporadic septicemia) of fattening pigs in Spain, and was provided by the Infectious Diseases Laboratory (Ref. 301/99) of the UAB. The oral inoculum was prepared by 24 h incubation at 37°C in buffered peptone water (BPW) (Oxoid; Hampshire, United Kingdom) and diluted (1:20) with sterile phosphate buffered saline (PBS) (Sigma–Aldrich; Madrid, Spain) to reach a final concentration of 2.5 × 108 cfu/mL.

Experimental Procedure

The duration of the study was 16 days, in which performance and clinical data were evaluated. After 1 week of adaptation to the diets (Day 8), a single 2 mL dose (5 × 108 cfu) of Salmonella Typhimurium was administered to the challenged animals by oral gavage and a single 2 mL dose of sterile BPW to the non-challenged animals (challenge control group).

Body weight was recorded on Days 1, 8, 12 and 16, while feed consumption was recorded on Days 1 and 7, and on a daily basis of the post-inoculation (PI) period (Days 8–16). The average daily gain (ADG), average daily feed intake (ADFI) and gain:feed ratio (G:F) were calculated by pen. Animals were checked daily for clinical signs to evaluate their status (i.e., dehydration, apathy and fecal score) after the Salmonella challenge, always by the same person. The fecal score was measured using a scale: 1 = solid and cloddy, 2 = soft with shape, 3 = very soft or viscous liquid, and 4 = watery or with blood. Rectal temperature was assessed with a digital thermometer (Thermoval Rapid, Hartmann; Spain) on Days 9 and 10 (1 and 2 PI). The mortality rate was also recorded, and no antibiotic treatment was administered to any of the animals of the experiment.

For microbiological analysis, on Day 1 fecal samples were taken aseptically from 24 animals that were randomly selected from the total before distribution. Samples were taken after spontaneous defecation associated with the manipulation of the animal or by digital stimulation. On Days 8, 9, 11 and 15 (Days 0, 1, 3 and 7 PI), fecal samples were taken from the animal with the highest initial BW of each pen (N = 24).

On Days 4 and 8 PI (Experimental Days 12 and 16, respectively), one pig per pen was euthanized. On Day 4 PI, the animal selected was the one with the intermediate initial BW, while on Day 8 PI the heaviest was selected.

Animals were euthanized and sequentially sampled during the morning (between 09:00 and 12:00 h). Prior to euthanasia, a 10 mL sample of blood was obtained by venipuncture of the cranial vena cava using 10 mL tubes without anticoagulant (Aquisel; Madrid, Spain). Immediately after blood sampling, selected piglets received an intravenous lethal injection of sodium pentobarbital (200 mg/kg body weight) (Dolethal; Vetoquinol S.A.; Madrid, Spain). Once dead, animals were bled, the abdomen was immediately opened and the whole gastrointestinal tract was excised.

Digesta (approximately 50 mL) from the ileum and proximal colon (considered to be 0.75 m from the ileocecal junction) was collected and homogenized. The pH of the digesta was determined immediately after homogenization of the samples with a pH-meter calibrated on each day of use (Crison 52–32 electrode, Net Interlab; Barcelona, Spain). Without delay, contents collected were sub-sampled and kept on ice until analysis or were stored. Colonic samples (1 g) were plated for Salmonella quantification. To determine the presence of the probiotic in the gut, 2 g of digesta were sampled (only on Day 8 PI) and bacterial isolation was performed before storing them at -80°C with GenIUL commercial protocol (Terrassa, Spain). Briefly, 1 g of colonic content sample was weighed in a 15 mL falcon and diluted 1:10 with enriched MRS broth (Oxoid; Madrid, Spain) + 0.25% cysteine (Sigma–Aldrich; Madrid, Spain) + 2% Tween 80 (Sigma–Aldrich; Madrid, Spain). Ten glass spheres (5 mm diameter) were added to the tube and vortex (1 min) to homogenize the suspension. Two-hundred and fifty microliter of the sample suspension were transferred to an eppendorf with 250 μL of enriched MRS broth. Three centrifugation (13,000 × g for 5 min at 4°C) and re-suspension (500 μL of enriched MRS broth) steps were performed, and finally the bacterial pellet was re-suspended in 200 μL of sterile PBS and stored at -80°C for DNA extraction and quantification via quantitative polymerase chain reaction (qPCR). A set of ileal and colonic digesta samples were preserved in a H2SO4 solution (3 mL of digesta plus 3 mL of 0.2 N H2SO4) for ammonia (NH3) determination, and were kept frozen at -20°C. An additional ileal and colonic sample set (approximately 20 g) was also frozen (-20°C) until analyzed for short-chain fatty acids (SCFA) and lactic acid.

For the histological study, 3 cm sections of the ileum were removed, opened longitudinally, washed thoroughly with sterile PBS and fixed by immersion in a 4% formaldehyde solution (Carlo-Erba Reagents; Sabadell, Spain).

Blood samples were centrifuged (3,000 × g for 15 min at 4°C) after 4 h refrigeration, and the serum obtained was divided into different aliquots and stored at -20°C to evaluate immune response.

Analytical Procedures

Chemical analyses of the diets including DM, ash, crude protein and diethyl ether extract, were performed according to the Association of Official Agricultural Chemists standard procedures (AOAC International, 1995). Neutral detergent fiber and ADF were determined according to the method of Van Soest et al. (1991).

For probiotic detection, DNA was extracted with a commercial kit following the manufacturer’s instructions (v-DNA reagent, Doc. Code 450000112.GenIUL; Terrassa, Spain). Briefly, samples were suspended in 1 mL of v-DNA buffer and centrifuged (13,000 × g for 5 min at 4°C). An incubation of the bacterial pellet (90°C, 10 min) with 200 μL of v-DNA reagent was performed in a shaking incubator and, finally, DNA was suspended in 600 μL of v-DNA buffer. The GenIUL Bifidobacterium spp. qPCR kit was used for probiotic quantification (reference: 4900021000, GenIUL; Terrassa, Spain). The kit provided a Bifidobacterium longum CECT 4551 DNA standard for the construction of standard curves (from 2 × 106 to 20 DNA copies per PCR reaction). Each reaction included 4 μl of a 5× HOT FIREPol qPCR Master mix including qPCR assay primers designed for the 16s RNA gene, 5 μl of diluted (1/10) DNA samples and 11 μl of RNAse free water. Reaction conditions for amplification of DNA were 95°C for 15 min and 45 cycles of 95°C, 15 s for denaturation, 54°C, 30 s for annealing and 72°C, 45 s for extension and fluorescent detection. To determine the specificity of the amplification, an analysis of the product-melting curve was performed after the last cycle of each amplification. The minimum level of detection of the method, considering the amount of DNA included in each reaction, was established at 6.3 × 103 16 S ribosomal RNA gene copies/g of fresh matter (FM) sample, compared to a non-template control dissociation curve. Real-time PCR was performed with the ABI 7900 HT Sequence Detection System (PE Biosystems) using optical-grade 96-well plates.

Ammonia concentration in digestive samples was determined with the aid of a gas-sensitive electrode (Hach Co., Loveland, CO, United States) combined with a digital voltmeter (Crison GLP 22, Crison Instruments, S.A.; Barcelona, Spain). Three grams of acidified content were diluted (1:2) with 0.16 M NaOH, after homogenization samples were centrifuged (1500 × g) for 10 min. The ammonia released was measured in the supernatants as different voltages in mV according to a procedure previously described in Hermes et al. (2009) that was adapted from Diebold et al. (2004). The SCFA and lactic acid analyses were performed by gas chromatography. The samples were submitted to an acid-base treatment followed by an ether extraction and derivatization with N-(tert-butyldimethylsilyl)-N-methyl-trifluoroacetamide (MBTSTFA) plus 1% tert-butyldimethylchlorosilane (TBDMCS) agent, using the method of Richardson et al. (1989), modified by Jensen et al. (1995). For Salmonella bacteria counts, all samples were transferred (1:10) to BPW. Quantitative assessment was made by seeding the 10-2, 10-4 and 10-6 serial dilutions of the samples in Xylose-Lactose-Tergitol-4 (XLT4) plates (Merck; Madrid, Spain). The qualitative assessment was made by incubating samples in BPW (37°C, 24 h), transferring them to Rappaport-Vassiliadis enrichment broth (Oxoid; Hampshire, United Kingdom) for a second incubation (42°C, 48 h), and finally seeding them in XLT4 plates in order to observe H2S-positive colonies.

Tissue samples for morphological measures were dehydrated and embedded in paraffin wax, sectioned to a 4 μm thickness and stained with hematoxylin and eosin. Measurements of 10 different villous-crypt complexes per sample were performed with a light microscope (BHS, Olympus; Barcelona, Spain) using the technique described in Nofrarías et al. (2006).

Serum concentrations of Tumor Necrosis Factor-α (TNF-α) were determined by Quantikine Porcine TNF-α kits (R&D Systems; Minneapolis, MN, United States) according to the manufacturer’s instructions. Pig major acute-phase protein (Pig-MAP) concentrations were determined by a sandwich-type ELISA (Pig MAP Kit ELISA, Pig CHAMP Pro Europe S.A.; Segovia, Spain) as described in Saco et al. (2011). Serological antibodies of Salmonella were tested by ELISA Salmonella Herdcheck (Idexx; Hoofddorp, Netherlands), and the cut-off for positivity was established at optic density ≥40%.

Statistical Analysis

Results are expressed as LS-Means with their standard errors unless otherwise stated. A two-way ANOVA was used to examine the effect of experimental challenge and probiotic treatment, as well as the interaction between the two (only included when significant). The general linear and mixed models of SAS (SAS Institute Inc., 2009) were used to analyze the effect of experimental treatments. For microbiological data, Fisher’s exact test was used to analyze the frequencies of positive animals as contingency tables, and the odds ratio (OR) with its 95% confidence interval was calculated on the basis of fixed effects.

When treatment effects were established, treatment means were separated using the probability-of-differences function adjusted by Tukey–Kramer. The pen was considered the experimental unit for analysis, and random effect was used to account for variation between pens. The α-level used for the determination of significance for all of the analysis was P = 0.05. The statistical trend was also considered for P < 0.10.

Results

In general, the trial proceeded as expected. Animals showed a good health status at the beginning of the experiment. None of the animals seeded Salmonella in feces on arrival, and serological analysis confirmed that animals had not been exposed to Salmonella previous to the day of inoculation, all animals being analyzed as seronegative along the whole trial. During the PI period, three deaths and an euthanasia for ethical reasons were registered in the challenged groups; one from the CN group the 4th day after inoculation and three from the CP group on Days 3, 5, and 6 PI, all from different pens. Necropsy was performed on the dead animals. All of them presented fibrinohemorrhagic gastritis and acute diffuse fibrinous enteric-tiflo-colitis, lesions normally associated with infection of Salmonella Typhimurium in pigs (Wilcock and Olander, 1977). Although casualties in the CP group were more than those in the CN group (3/24 vs. 1/24), differences were not statistically significant. No antibiotic treatment was administered to any of the animals in the trial.

The ability of the probiotic strains to colonize the gut was indirectly evaluated by analyzing the total Bifidobacterium spp. copies in the colonic content on Day 8 PI. Mean concentrations of DNA copies/g of FM detected were 3.16 × 107 for CN, 2.22 × 107 for CP, 2.03 × 107 for NN, and 8.11 × 107 for NP. Probiotic and challenge effects were not significant, but a tendency was seen for the interaction challenge × probiotic (P = 0.058), where the number of DNA copies increased only in non-challenged animals receiving the probiotic.

Animal Performance

Effects of the experimental treatments on BW, ADG, and ADFI are expressed in Table . The Salmonella challenge negatively affected final BW, ADFI, and ADG in the post-challenge period.

Changes in Fermentative Activity

Table shows the changes promoted by the experimental treatments on the main ileal and colonic fermentation products.

Probiotic treatment did not show significant effects on the studied parameters despite a tendency to interaction (P = 0.063) seen for the ADG before the challenge, the CP group showing a higher ADG than did its control (CN).

Evolution of ADFI during the post-challenge period is shown in Figure . Feed intake was reduced by the Salmonella challenge (P < 0.001), this effect being especially manifested on Day 1 post-inoculation (interaction challenge × day P = 0.034). A tendency was found for the probiotic to enhance feed consumption (P = 0.069), and although not significantly, this effect was more manifested in the inoculated animals (interaction challenge × probiotic P = 0.078).

Average daily feed-intake evolution along the post-inoculation (PI) period. Treatments: CN, challenged + no probiotic; CP, challenged + probiotic; NN, no challenge + no probiotic; NP, no challenge + probiotic. n = 8 for groups CN and CP, n = 4 for groups NN and NP. Interactions only included when significant. Bars represent the standard error of the LS-Means.

Clinical Signs

Figure shows the evolution of fecal consistency after the challenge. Salmonella inoculation significantly affected fecal scores with more liquid feces (P challenge < 0.001), especially from Day 3 onwards (P challenge × day = 0.035). Administration of the probiotic improved fecal consistency, with decreases in the fecal score in both challenged and non-challenged animals (P = 0.014).

Evolution of the mean fecal scores in the different experimental groups along the post-inoculation (PI) period. Fecal score was measured using a scale from 1 (solid and cloddy) to 4 (watery or with blood). Treatments: CN, challenged + no probiotic; CP, challenged + probiotic; NN, no challenge + no probiotic; NP, no challenge + probiotic. n = 8 for groups CN and CP, n = 4 for groups NN and NP. P-values only included when significant. Bars represent the standard error of the LS-Means.

On Day 1 PI, the challenged animals presented significantly higher rectal temperatures than did the non-challenged animals (40.0°C vs. 39.3°C, P < 0.001) despite the administration of the probiotic. However, on Day 2 PI, only the challenged animals not receiving the probiotic presented higher temperatures (39.9°C vs. 39.2°C, 39.1°C and 38.9°C for CN, CP, NN, and NP, respectively) (P interaction probiotic × day = 0.048).

Salmonella Analysis

None of the analyzed animals seeded Salmonella on arrival. Figure shows the prevalence of positive animals to Salmonella during the post-challenge period. After the oral challenge with Salmonella, all animals except one that received the bacterial inoculum were positive in feces and stayed positive for all of the remaining experimental period. Unexpectedly, three animals were positive for Salmonella before inoculation (Day 0 PI), and some additional animals of the non-challenged group also became positive for Salmonella on Days 1, 3, 4, 7, and 8 PI. However, from all samples analyzed in the PI period, 98.7% of the samples of challenged animals were found to be positive (1–102 cfu/g) during the PI period, while only 45% of the samples of non-challenged animals were positive. No significant effects were seen with the probiotic.

Percentage of positive (>1 cfu/g) animals to Salmonella spp. in feces (Day 0, Day 1, Days 3, and 7 post-inoculation [PI]) or colonic content (Days 4 and 8 PI). Treatments: CN, challenged + no probiotic; CP, challenged + probiotic; NN, no challenge + no probiotic; NP, no challenge + probiotic. n = 8 for groups CN and CP, n = 4 for groups NN and NP.

Figure represents the semi-quantitative analysis of Salmonella in feces and colon digesta of those animals that received the pathogen inoculum. None of the non-challenged animals excreted Salmonella in quantifiable levels (>102 cfu/g) and, therefore, they are not represented in the figure. The probiotic administration significantly lowered the number of animals with high Salmonella excretion levels on Day 1 (P = 0.028) and also tended to lower them on Days 3 (P = 0.078) and 4 (P = 0.056), with an increase in the frequency of the animals with less than 103 cfu/g.

Number of animals in the different range levels of Salmonella spp. in feces (Days 1, 3, and 7 post-inoculation [PI]) or colonic digesta (Days 4 and 8 PI). Range Levels: Negative (0 cfu/g), Very low (1–102 cfu/g), Low (103–104 cfu/g), High (105–106 cfu/g) and Very high (107–108 cfu/g). CN (challenged + no probiotic) and CP (challenged + probiotic). n = 8 for groups CN and CP (except n = 7 for CP on Day 8 PI).

In the ileum, the Salmonella challenge caused a mild affection with a tendency to decrease ileal, lactic acid concentrations on Day 4 PI (P = 0.096) and to increase pH on Day 8 PI (P = 0.099). The colon was more severely affected, with a significant (P < 0.001) decrease in lactic acid concentrations on Day 8 PI and numerical decreases on Day 4 PI (P = 0.141). Significant decreases of colonic SCFA were also observed on Day 4 PI (P = 0.030) together with a tendency to increase ammonia concentrations (P = 0.104) on Day 8 PI.

Some beneficial changes were observed in the fermentation profile with the probiotic treatment. A significant increase in ileal acetic acid (P = 0.008) was seen on Day 8 PI, this increase being of a bigger magnitude in non-challenged animals (P challenge × probiotic = 0.097). Moreover, a tendency to decrease colonic ammonia concentrations (P = 0.078) was detected on Day 8 PI. Some changes promoted by the probiotic were not the same in challenged and non-challenged animals. Surprisingly, increased ileal ammonia levels were detected in the NP group, while a decrease was observed in CP animals in comparison to their control (P challenge × probiotic = 0.016). A trend for a similar pattern was observed for pH in the colon on Day 8 PI (P challenge × probiotic = 0.058). On the other hand, a tendency to decrease colonic total SCFA in the NP group and increase them in the CP group was seen on Day 8 PI (P challenge × probiotic = 0.057). Molar ratios of colonic SCFA were not significantly modified by any of the treatments; mean molar ratios detected in the trial were 62.7% acetic, 23.6% propionic, 9.8% butyric, 3.0% valeric and 1.1% branched-chain fatty acids.

Immune Response

Table reports the serological concentrations of acute-phase proteins Pig-MAP and the pro-inflammatory cytokine TNF-α. The Salmonella challenge caused significant (P < 0.05) increases in both indexes, except on Pig-Map, on Day 8 PI, where the increase was numeric (P = 0.140). No significant effects were observed with the probiotic treatment although a numeric decrease of TNF-α was observed on Day 8 PI (P = 0.121) in animals receiving the probiotic treatment.

Intestinal Morphology

The histomorphological results of the ileum are summarized in Table . The challenge with Salmonella caused important decreases in villous height (P = 0.026 on Day 4; P = 0.061 on Day 8 PI), and although the crypt depth was not affected, the challenge significantly altered the villus:crypt ratio both days (P < 0.05). Additionally, an increase was seen in the number of goblet cells (GC) on Day 8 PI (P = 0.018) and on the number of mitosis on Day 4 PI (P = 0.022).

Probiotic administration promoted a different effect on challenged and non-challenged animals. Whereas the probiotic moderately increased villous height in the challenged animals, it decreased it in the non-challenged ones (Day 8 PI; P challenge × probiotic = 0.038). Regarding crypts, the probiotic increased the crypt depth of the non-challenged animals until levels similar to the challenged ones (Day 8 PI; P challenge × probiotic = 0.011). These changes were reflected in the villous:crypt ratio (Day 8 PI; P challenge × probiotic < 0.001). Intraepithelial lymphocytes (IEL) were significantly increased by the probiotic on Day 8 PI in both groups (P = 0.015).

Discussion

The aim of this study is to determine if the administration of the probiotic combination of B. infantis IM1® and B. lactis BPL6 conferred protection against Salmonella Typhimurium.

A 2-week trial using weanling piglets was performed, where animals were challenged with Salmonella after 7 days of adaptation to the treatments and new environment. The challenge promoted an acute episode of diarrhea with increased fecal scores, fever response and the death (natural or euthanasia) of four animals that presented fibrinous-hemorrhagic lesions, normally associated with Salmonella Typhimurium (Wilcock and Olander, 1977). Virtually all parameters studied responded significantly to the pathogen inoculation: performance parameters, fermentation products, inflammatory response and ileal histomorphology were severely altered in comparison to non-challenged controls.

The administration of the probiotic combination was not able to prevent the infection of the animals by Salmonella, as mostly all of them became positive in feces 1 day after the challenge. Despite this, the probiotic was able to reduce the pathogen load in colon and feces, suggesting the potential of the bifidobacteria combination to exclude Salmonella. In this sense, it is also interesting to comment that, in our study, we unexpectedly found some animals becoming positive to Salmonella in feces in the non-challenged groups during the PI period, despite the seeding levels being very low (<102 cfu/g). This can be attributed to some failure in the biosecurity protocol, as low concentrations of Salmonella in the environment (102 to 103 cfu) have been reported as being able to infect exposed animals (Hurd et al., 2001; Boughton et al., 2007). The fact that all fecal samples were negative for Salmonella on their arrival, and that all euthanized piglets remained seronegative at the end of the study, reaffirms that these animals were not previously exposed to the pathogen in the farm of origin (Nielsen et al., 1995). In those animals, it is interesting to point out that although all NN animals were positive in 2 days PI, the maximum percentage of positive animals for NP was 50% during all of the PI week. This could suggest that, although the probiotic was not able to prevent the infection of the animals when they were exposed to a high oral load of Salmonella, it could have some effect in front of a low exposure maintained over time. However, protection in our experiment was not significant, probably due to the low number of replicates in non-challenged animals (n = 4).

In vitro studies have shown the ability of bifidobacteria to inhibit the growth of Salmonella (Bielecka et al., 1998; Tanner et al., 2016). A pluripotent stimulatory effect on the immune system (Gill et al., 2001; Medina et al., 2007; Akahashi et al., 2013), production of organic acids (Saulnier et al., 2009), production of bacteriocins and bacteriocin-like substances (Cheikhyoussef et al., 2008), and the capacity to inhibit the pathogenic adhesion to enterocytes or prevent bacterial translocation (Gagnon et al., 2004; Searle et al., 2009) have been described as the possible mechanisms of action of Bifidobacterium spp. for these antimicrobial effects. Regarding the strains evaluated in this study, previous works using a similar model of disease have also demonstrated the potential of the B. infantis IM1® strain to reduce Salmonella loads (Barba-Vidal et al., 2017). For this B. infantis IM1® strain, several mechanisms have been reported that could be involved in a favorable outcome: the potential to produce peptides with protease activity (Chenoll et al., 2016), immunomodulatory capacity by increasing IL-10 (unpublished data) and IgA (Moreno Muñoz et al., 2011) production have been reported.

In accordance with reductions in the pathogen loads, improvements in clinical parameters were also registered with the probiotic combination. Rectal temperature of the CP group returned to levels similar to those of the non-challenged groups 48 h after the pathogen inoculation, and fecal scores showed less diarrhea. Regarding diarrhea scores, it is also interesting to remark that they were reduced not only in the CP group but also in the NP group. After weaning, piglets suffer stress for several abrupt changes: separation from the sow, change from a milk-based to a less-digestible dry-cereal-based feed diet, introduction to new social partners and new physical environments (Weary et al., 2008), which usually promote gut dysbiosis. Our results suggest that the probiotic treatment may not only improve piglet outcome against pathogens, but it may also help piglets in a post-weaning period.

Differences in productive parameters are rarely reported in challenge trials evaluating probiotic treatments, as these studies are usually run in short periods and with a limited number of animals. Despite this, we were able to see trends for a positive effect of the probiotic in the intake of feed during the post-challenge period, more manifested in the CP group, and also a numerically higher final live-weight (P = 0.131) in the animals receiving the probiotic, with more than 500 g of difference at the end of the study. In this study, this increase in feed intake and weight should be considered as a sign of better health status and adaptation to the weaning stress that allows the animal to express its genetic growth potential. These positive results should not be considered as a risk for obesity, as has clearly been stated by Bernardeau and Vernoux (2013) for the extrapolation of farm-animal results to humans.

Modulation of the fermentation profile was also detected with the probiotic treatment at the ileal and colonic level. A general increase in ileal acetic acid concentrations (more importantly in the NP group) was registered on Day 8 PI. Scientific literature reports that carbohydrate degradation by bifidobacteria exclusively takes place by the characteristic fructose-6-phosphate shunt (or bifidus pathway). Acetic acid and lactic acid are the major end-metabolites (de Vries and Stouthamer, 1967; Van der Meulen et al., 2006), with a theoretical molar ratio of acetic acid to lactic acid of 1.5 (de Vries and Stouthamer, 1968; Van der Meulen et al., 2006). Considering this, we speculate that increases in acetic acid could be due to a higher bifidobacterial presence in the ileum in animals treated with probiotic although we cannot discard other bacterial species to be involved too. Lactic acid, as the main product of most of the inhabitants of the small intestine (Clemens and Stevens, 1979), would not have been sensitive enough to reflect changes. This increase in acetic acid was more manifested in non-challenged animals on Day 8 PI, reflecting a more established ileal microbiota at this time. Actually, on Day 8 PI, we were also able to detect a higher number of Bifidobacterium spp. in the colon by qPCR quantification in the non-challenged animals receiving the probiotic. However, changes in ileal fermentation were not always favorable. An interaction effect increasing ileal ammonia concentrations in NP and decreasing in CP was observed on Day 4 PI. We cannot find an explanation for this; however, it is worth mentioning that this effect disappeared on Day 8 PI with a substantial reduction in ammonia mean values for all treatments. This evolution in ileal ammonia could be a reflection of the big transitions of microbial populations that are produced during first days after weaning (Wang et al., 2013), regardless of the experimental treatment the animals received.

In relation to colonic fermentation, some benefits related to the probiotic were observed on Day 8 PI. Firstly, a reduction in ammonia concentration was reported (P = 0.078). This effect could be due to the ability to utilize ammonia attributed to bifidobacteria or an indirect effect via modulation of the fermentation profile (Arunachalam, 1999; Ahasan et al., 2015) with a reduction in the proteolytic populations. Secondly, an interaction in SCFA on Day 8 PI was observed. The concentration increased in CP groups to levels similar to those of the NN group and could suggest a normalization of the fermentative activity with the probiotic in challenged animals. Nevertheless, SCFA were decreased by the probiotic in the non-challenged group. This reduction would be generally accepted as a negative impact of the probiotic on gut health. However, in our case it can also be a natural consequence of a reduced amount of fermentable substrates arriving in the colon. The abrupt increase observed for acetic acid in the ileum of these animals could suggest a more active microbial population at the end of the small intestine that could have reduced the amount of substrates susceptible to be fermented in the colon. Differentially to humans, the fermentative activity at the end of the small intestine in pigs is quite important.

Interesting results were also observed for ileal histomorphometry on Day 8 PI. Whereas the probiotic treatment maintained villous height of challenged animals to similar levels as of non-challenged, numerical reductions in the NP group were observed. Moreover, in the non-challenged animals the probiotic also promoted an increase in crypt depths up to similar values of the challenged animals. Subsequently, changes were reflected accordingly in the villous:crypt ratio. These results could again be related to a higher colonization of the ileum by the probiotic bacteria and to the presence of a greater ileal fermentative activity in these animals. In consonance, Kleessen et al. (2003) observed increased jejunal villus height and crypt depth in a rat model of human fecal microbiota due to fermentation of fructans by bifidobacteria. It is also important to keep the great capacity to adhere to enterocytes reported for bifidobacteria in mind (Servin, 2003; Collado et al., 2005, Collado et al., 2007a), which has been reported to be increased in combination of probiotic strains including Bifidobacterium spp. (Collado et al., 2007a). We suspect that the presence of highly adhesive bifidobacteria could have contributed to the exclusion of intestinal pathogens (Collado et al., 2005) in challenged animals, as the CN group had a more severely affected villous height. However, the adhesion of these bifidobacteria in the non-challenged animals, and the increased fermentative activity observed in the ileum, could have somehow compromised villous enterocytes in the NP group. To our knowledge, it is the first time that such a reduction on villous height has been described due to a bifidobacterial probiotic. Still, similar results were also found for this probiotic combination by our group in other non-published studies, proving that these effects are quite consistent. Nevertheless, none of the parameters analyzed in this study suggests negative effects of the probiotic in this group, and TNF-α showed the lowest values in them, suggesting no deleterious effects on the intestine. Interestingly, IEL mean values were decreased between Days 4 and 8 PI only in the animals not receiving the probiotic, despite their being challenged or not with Salmonella. Possibly the increased values observed on Day 4 were due to opportunistic pathogens taking advantage of a transient dysbiosis related to weaning. On Day 8, only the animals receiving the bifidobacteria maintained those response levels, suggesting the ability of the probiotic strains to stimulate the immune system of the animal.

Bifidobacteria are considered to be minor colonizers of swine gut post-weaning (Konstantinov et al., 2004; Zhao et al., 2015). Colonic concentrations of Bifidobacterium spp. reported in the piglet colon range from 105 to 108 cfu/g (Mountzouris et al., 2006; Fouhse et al., 2015), and Mountzouris et al. (2006) estimated that they contribute to approximately 0.4 ± 0.15% of total bacteria in the ascending colon. In our study, total Bifidobacterium spp. was analyzed via qPCR and, despite a 109 daily dose of combined Bifidobacteria being used, noticeable increases were only observed in the non-challenged animals. Low detection levels in the challenge animals could respond to the gut dysbiosis produced by the Salmonella challenge that had precluded the probiotic to fully colonize the gut. Furthermore, it should be considered that at the moment the samples were taken, the animals had not received the probiotic in the previous 24 h. Therefore, considering that transit time is accelerated in intestinal disorders, unless the probiotic strains had colonized the gut, it would have been very improbable to detect it in the colonic samples. The lack of response of the qPCR numbers for Bifidobacterium spp. also could respond to a substitution between species, maintaining the niche a similar size. For this reason, although we cannot demonstrate the colonization of the gut by the probiotic strains, it cannot be discarded either. Even in the eventual case of the strains not colonizing the gut, another possible explanation for the effects observed with the probiotic could be that effects were mediated by metabolic products or other bioactive compounds and not by the bacteria cells themselves. In this regard Bifidobacterium infantis immunomodulation seems to be at least partially regulated by bioactive peptides which can retain their biological activity even without the strain being present (Ewaschuk et al., 2008). In this line, a recent publication demonstrates that one of the strains included in this combination, B. infantis IM1®, produces peptides with protease activity (Chenoll et al., 2016).

As it could be seen, the probiotic combination evaluated in this study has demonstrated a clear positive effect, not only ameliorating the Salmonella challenge outcome but also improving weaning response. These results are better than previous ones obtained by our group for the B. infantis IM1® single strain (Barba-Vidal et al., 2017) with a similar experimental design. In that study, the use of the B. infantis IM1® strain also diminished Salmonella shedding, although challenged animals treated with the probiotic failed to show the significant improvements observed in this study in clinical outcomes, fermentation or histomorphometry. Other authors have also described the benefits of using a combination of different strains (Perdigon et al., 1990; Casey et al., 2007). However, unfortunately, in vivo studies comparing the effect of single strains with the strain combination are still rare (Chapman et al., 2011). In our study, the reported results suggest that the evaluated combination of bifidobacterial strains showed a better outcome that results previously reported for the single strain B. infantis IM1® (Barba-Vidal et al., 2017). However, our experimental design does not allow us to identify if the reason for this improvement is due complementary effects of the strains, as both strains were not tested individually in this study.

Conclusion

The probiotic combination of B. infantis IM1® and B. lactis BPL6 had a positive effect on enhancing gut health on post-weaning piglets and alleviating animals in a Salmonella challenge. Improvements registered in challenged animals were a reduction of the fecal excretion of Salmonella Typhimurium, a decrease in rectal temperature to similar levels to that in non-challenged animals and improvements in the villous:crypt ratio. In addition, general probiotic benefits were observed in both challenged and non-challenged groups, showing an increase in voluntary feed-intake, a decrease of diarrhea scores, healthier fermentation profiles and a stimulation of the intestinal immune system by increasing IEL.

Author Contributions

EB-V participated in the experimental design, was responsible for the animal trial, laboratory analysis, data analysis, and writing. LC participated in the experimental design, animal trials, data analysis and writing. VR participated in animal trials, data analysis, and writing. GC-O and JM participated in the experimental design, contributed to data analysis, and writing. SM-O participated in the experimental design, animal trials, laboratory analysis, data analysis, and writing.

Conflict of Interest Statement

This work was partially funded by Laboratorios Ordesa. GC-O and JM are employees of Laboratorios Ordesa S.L. The others 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

Table 1

Ingredient composition and nutrient analysis of the experimental diets as-fed basis, g/kg.

Ingredients
Maize	280.7
Wheat	170.0
Barley	150.0
Extruded soybean	122.4
Sweet whey-powder	100.0
Fishmeal LT	50.0
Soybean meal 44	50.0
Whey-powder 50% fat	30.3
Mono-calcium phosphate	21.3
Calcium carbonate	8.2
L-Lysine HCL	4.5
Vitamin-Mineral Premixa	4.0
Sodium chloride	3.0
DL-Methionine 99	2.4
L-Threonine	2.3
L-Tryptophan	0.9
Chemical composition
DM	903.2
Ash	74.1
Crude fat	64.5
Crude protein	189.3
Neutral detergent fiber	111.6
Acid-detergent fiber	35.1

Table 2

Animal performance parameters.

	Treatmentsa				P-value
	CN	CP	NN	NP	RSDb	Challenge	Probiotic	Interaction
BWc (kg)
Initial	7.90	7.51	7.60	7.85	0.559	0.929	0.770	0.195
Final	8.78	9.34	9.82	10.35	0.834	0.010	0.131	0.967
ADFId (g/d)
Pre-inoculatione	259	306	273	250	55.9	0.391	0.611	0.164
Post-inoculationf	240	343	435	445	114.9	0.008	0.276	0.368
ADGg (g/d)
Pre-inoculatione	53	119	78	58	50.5	0.417	0.303	0.063
Post-inoculationf	13	97	273	300	122.5	<0.001	0.309	0.601

Table 3

Colonic pH values, ammonia concentration and fermentation products for Days 4 and 8 post-inoculation (PI).

		Treatmentsa				P-value
	Days PI	CN	CP	NN	NP	RSDb	Challenge	Probiotic	Interaction
Ileum
pH	4	6.85	6.76	6.56	6.80	0.539	0.608	0.751	0.515
	8	6.83	6.76	6.66	6.28	0.409	0.099	0.239	0.419
NH3 (mmol/L)	4	4.47	2.37	2.95	5.13	1.77	0.455	0.961	0.016
	8	0.81	0.71	1.09	0.74	0.648	0.581	0.425	0.651
Acetic acid (mmol/kg)	4	2.58	5.06	3.03	3.95	4.280	0.887	0.403	0.706
	8	2.73	3.89	1.60	6.15	2.210	0.568	0.008	0.097
Lactic acid (mmol/kg)	4	19.8	37.0	54.4	58.6	34.74	0.096	0.515	0.691
	8	49.1	45.7	22.6	43.1	36.72	0.376	0.602	0.466
Colon
pH	4	6.19	6.07	5.77	6.03	0.476	0.275	0.758	0.379
	8	6.14	5.96	5.82	6.11	0.254	0.473	0.626	0.058
NH3 (mmol/L)	4	6.59	5.71	4.89	5.62	4.398	0.643	0.967	0.678
	8	7.82	5.38	5.54	4.11	2.370	0.104	0.078	0.635
SCFAc (mmol/kg)	4	98.4	94.1	136.2	138.5	39.42	0.030	0.957	0.853
	8	115.0	140.7	140.3	123.0	24.27	0.724	0.695	0.057
Lactic acid (mmol/kg)	4	1.00	4.82	5.10	8.43	5.644	0.141	0.170	0.923
	8	0.84	1.01	12.07	8.07	4.699	<0.001	0.363	0.324

Table 4

Effects on serum levels of pro-inflammatory cytokine TNF-α and acute-phase protein Pig-MAP on Days 4 and 8 post-inoculation (PI).

	Treatmentsa				P-value
	CN	CP	NN	NP	RSDb	Challenge	Probiotic	Interaction
Pig-Map (mg/ml)
Day 4 PI	3.38	2.31	1.03	1.10	1.657	0.024	0.504	0.446
Day 8 PI	2.31	1.57	1.45	1.05	1.019	0.140	0.215	0.708
TNF-α (pg/ml)
Day 4 PI	151	158	87.7	77.6	41.30	<0.001	0.927	0.647
Day 8 PI	112	82.6	63.9	61.6	21.95	0.002	0.121	0.182

Table 5

Ileal histomorphometry on Days 4 and 8 post-inoculation (PI).

		Treatmentsa				P-value
	Days PI	CN	CP	NN	NP	RSDb	Challenge	Probiotic	Interaction
Villous height (μm)	4	192.0	183.6	258.1	256.9	65.94	0.026	0.869	0.903
	8	198.3B	243.4A,B	303.3A	237.5A,B	56.80	0.061	0.682	0.038
Crypt depth (μm)	4	253.9	249.2	225.6	268.1	27.24	0.696	0.125	0.059
	8	242.5A	242.7A	182.8B	259.1A	30.70	0.124	0.010	0.011
Villous:Crypt ratio	4	0.78	0.75	1.15	0.96	0.280	0.027	0.382	0.509
	8	0.81B	1.01B	1.67A	0.93B	0.218	<0.001	0.011	<0.001
IELc (N° cel/100 μm)	4	1.04	1.25	1.38	1.49	0.546	0.243	0.506	0.822
	8	0.73	1.21	0.98	1.44	0.398	0.178	0.015	0.950
GCd (N° cel/100 μm)	4	0.74	0.69	0.71	0.66	0.308	0.817	0.719	0.965
	8	0.96	1.04	0.66	0.44	0.401	0.018	0.697	0.402
Mitosise (N° cel/100 μm)	4	0.42	0.36	0.26	0.26	0.123	0.022	0.579	0.579
	8	0.25	0.26	0.34	0.20	0.097	0.765	0.150	0.103