Abstract
Tryptophan (Trp) plays an essential role in pig behavior and growth performances. However, little is known about Trp’s effects on tight junction barrier and intestinal health in weaned pigs. In the present study, twenty-four (24) weaned pigs were randomly assigned to one of the three treatments with 8 piglets/treatments. The piglets were fed different amounts of L-tryptophan (L-Trp) as follows: 0.0%, 0.15, and 0.75%, respectively, named zero Trp (ZTS), low Trp (LTS), and high Trp (HTS), respectively. No significant differences were observed in average daily gain (ADG), average daily feed intake (ADFI), and gain: feed (G/F) ratio between the groups. After 21 days of the feeding trial, results showed that dietary Trp significantly increased () crypt depth and significantly decreased () villus height to crypt depth ratio (VH/CD) in the jejunum of pig fed HTS. In addition, pig fed HTS had higher () serum diamine oxidase (DAO) and D-lactate. Furthermore, pig fed HTS significantly decreased mRNA expression of tight junction proteins occludin and ZO-1 but not claudin-1 in the jejunum. The number of intraepithelial lymphocytes and goblet cells were not significantly different () between the groups. Collectively, these data suggest that dietary Trp supplementation at a certain level (0.75%) may negatively affect the small intestinal structure in weaned pig.
1. Introduction
The postweaning period represents a delicate transitional phase in pig’s life. The numerous stresses to their endocrinology, metabolism, and physiology that piglets experience following weaning are reflected in homeostatic changes to their bodies. The gastrointestinal tract is particularly responsive to stressors. Weaning is known to compromise the digestive, absorptive, and secretory capacity of the small intestine which can cause morphological and histological changes of the small intestine [1–4]. In addition, weaning induces a deleterious effect on intestinal barrier function [5, 6].
Tryptophan has a potential role to facilitate stress adaptation of animals and human through increasing hypothalamic serotonin (5-hydroxytryptamine, 5-HT) level [7, 8]. Several studies have shown that dietary Trp may reduce stress hormone [7, 9, 10], reduce aggressive behaviors [11], and improve growth performance [8] in weaned pigs. As the precursor of serotonin, tryptophan is also known to play an essential role in the regulating several physiological function, such as motility (in duodenal and ileal), secretion and sensitivity [12], and intestinal permeability [13, 14] in the gastrointestinal tract. However, little is known about the effect of dietary Trp on intestinal epithelial cells growth and health, as well as intestinal epithelial tight junction proteins in weaned piglets [7, 15] (Table 5). This study was designed to evaluate the effects of dietary Trp on intestinal epithelial morphology and mRNA level of tight junction proteins in weaned pig.
2. Materiel and Methods
2.1. Experimental Animals and Diets
The study was approved by the Animal Care and Use Committee of the Chinese Academy of Sciences and performed according to the Chinese Guidelines for Animal Welfare. This animal experiment was conducted at technology innovation platform for national research institutions located in Hunan province “Experimental Station for Healthy Production of Livestock and Poultry & Environmental Control.” Thirty-six healthy piglets of similar body weight ( kg) (landrace large white) from different litters were obtained from a local farm and transported to the experimental site of the Institute of Subtropical Agriculture. Piglets were weighed and allocated to individual pens in the same room. The piglets were fed mash feed. Diets were formulated to approximately meet or exceed the nutrient requirements of growing pigs as suggested by NRC 2012 [16]. The isonitrogenous diets were formulated and supplemented with different amounts of L-tryptophan (L-Trp) as follows: 0.0%, 0.15, and 0.75%, respectively, named zero Trp (ZTS), low Trp (LTS), and high Trp (HTS). All of the diets were based on corn and soybean meal. Proteins from whey powder and fishmeal were kept constant. The diets were balanced for the same level of crude protein. The compositions of the diets are shown in Table 1.
The piglets were housed individually in an environmentally controlled nursery with hard-plastic slatted flooring. The piglets were exposed to a 3-day adaptation period before being allocated to one of three dietary treatments. For 21 days, the piglets were given ad lib access to water and their respective diet. Each day, surplus feed and waste were collected and weighed. This was then dried at 100°C for several hours and weighed again to determine the initial dry matter content and calculate the feed intake. Each piglet’s body weight was monitored weekly. The feed conversion rate was calculated from the body weight and feed intake data.
2.2. Sample Collection
At day 22, after pigs were feed-deprived overnight, approximately 10 mL of blood was collected from jugular vein and serum samples were obtained by centrifugation at 2,000 g for 10 min at 4°C. These samples were immediately stored at −80°C for amino acids, D-lactase, and diamine oxidase determination. After blood sample collection, pigs were euthanized by electrical stunning and exsanguination. The gastrointestinal tract was removed and immediately dissected, with the small intestine being divided at the duodenum, jejunum, and ileum. Using sterile instruments, approximately 20 cm of intestinal tissue was removed from the center of each of these sections. Tissue samples were flushed with ice-cold saline to recover mucosa, yielding approximately 5 g from each tissue. The mucosa samples were straightaway frozen in liquid nitrogen and stored at –80°C until RNA was ready to be collected. To determine the morphology of the small intestine mucosa and to evaluate the proliferation of crypt cells, a 2 cm segment from each small intestine section was cut and fixed in 4% formaldehyde.
2.3. Intestinal Morphology and Crypt Cell Proliferation
Samples of the duodenum, jejunum, and ileum were fixed in formalin and then embedded in paraffin. Using a microtome, cross sections of the samples were cut to an approximate thickness of 5 μm and stained with haematoxylin and eosin. For each section, the density of goblet cells and lymphocytes together with the height of the villus (VH) and depth of crypts (CD) was calculated using computer-assisted microscopy (Nikon, ECLIPSE E200, Tokyo, Japan). To assess VH and CD consistently, measurements were made of the distance between the tip of the villus to the mouth of the crypt (VH) and the crypt mouth to the crypt base (CD). The ratio of VH to CD (VH/CD) was determined.
2.4. Serum Large Neutral Amino Acids Analysis
The serum obtained from the blood samples was used for large neutral amino acids determination. Isotope dilution liquid chromatography-tandem mass spectrometry was used to analyze serum amino acids. Analysis was conducted by Beijing Amino Medical Research Co., Ltd., Beijing, China.
2.5. Serum D-Lactate and Diamine Oxidase Levels in the Plasma
Serum D-lactate content was measured by a commercial kit (Sino-German Beijing Leadman Biotech Ltd., Beijing, China) and Beckman CX4 Chemistry Analyzer (Beckman Coulter, Brea, CA). The activities of the serum diamine oxidase were determined using kits according to the user’s manual (Nanjing Jiancheng Bioengineering Institute, Nanjing, China).
2.6. Relative Quantification of mRNA Expression
The abundance of occludin, zonula occludens-1 (ZO-1), and mRNA in the ileal mucosa was determined by RT-PCR.
TRIzol reagent (Invitrogen, Carlsbad, CA, US) was used in accordance with the manufacturer’s instructions to isolate RNA from the sample of liquid nitrogen-pulverised ileal mucosa. To ensure the integrity of the RNA, it was checked using 1% agarose gel electrophoresis and 10 μg/mL ethidium bromide stain. The quantity and quality of the RNA were analyzed by UV/Vis spectroscopy using a spectrophotometer (NanoDrop ND-1000; Thermo Fisher Scientific, Germany).
Complementary DNA (cDNA) was synthesised using 5x PrimeScript Buffer 2 and PrimeScript reverse transcriptase Enzyme Mix 1 (Takara Biotechnology (Dalian) Co., Ltd., Dalian, China). To assess gene expression, the ensuing cDNA was diluted and used as a PCR template. The reaction was carried out in 10 μL of PCR solution (ABI Prism 7700 Sequence Detection System); quantitative PCR (qPCR) analyses were conducted (ABI 7900HT Fast Real-Time PCR System; Applied Biosystems, Carlsbad, CA, USA) using 5 μL SYBR Green mix, 1 μL cDNA (diluted 4), 0.2 μL each of forward and reverse primers (details available in Table 2), 3.6 μL H2O, and 0.2 μL ROX Reference Dye (50x). Samples were exposed to predenaturation of 10 s at 95°C followed by 40 cycles of amplification; each cycle consisted of 5 s at 95°C and 20 s at 60°C. This was followed by a melting curve stage of a heating rate of 0.1°C/s−1 and melt temperature of 60°C to 90°C. GADPH was used as the reference gene. The relative expression of mRNA was calculated for the treatment and control groups as a ratio of target genes to GAPDH using , where ΔΔCt is the difference between of the treatment condition and of the control condition.
2.7. Statistical Analysis
All statistical analysis was performed using the Analysis of Variance (ANOVA) with the comparison of means by Duncan’s Multiple Comparison Test using IBM SPSS statistics version 22. A value less than 0.05 was considered to be significant.
3. Results
3.1. Growth Performance
The growth performance is presented in Table 3. No significant differences () were observed among treatments in daily gain, feed intake, and gain/feed. However, ADG was numerically improved by 8% and 11% during d7–d14 and 16% and 36% during d14–d21, respectively, by low Trp supplementation (LTS) and high Trp supplementation Trp (HTS) compared to zero Trp supplementation (ZTS).
3.2. Plasma Large Neutral Amino Acids
Table 4 showed that dietary Trp supplementation significantly increased () Trp and Trp/LNAA (large neutral amino acids) concentration in the plasma from the pig fed LTS and HTS compared with those fed ZTS. The concentration of valine (Val) and isoleucine (Ile) significantly decreased () in plasma from pig fed dietary Trp but Leu (leucine), Tyr (tyrosine), and Phe (phenylalanine) were the same between control and treatment groups.
3.3. Effect of Tryptophan on Pig Intestinal Morphology
The morphology of the duodenum, jejunum, and ileum at 21 days of the experiment is shown in Table 4.
The results showed that pig fed HTS significantly increased () CD and decreased VH/CD () in the jejunum compared to ZTS and LTS. No significant differences () were observed for villi height between groups.
3.4. Effect of Trp on Intestinal Barrier Function
The effect of dietary Trp on serum DAO activity and D-lactate content is shown in Table 6. There was no significant increase in serum DAO and D-lactate levels between the control and LTS group. Pig fed HTS had significantly increased DAO and D-lactate level compared to ZTS and LTS.
As shown in Figure 1, HTS significantly decreased mRNA level of occludin and ZO-1 in the jejunum of pig fed HTS compared to LTS and ZTS. mRNA expression of claudin-1 was the same between the groups.
4. Discussion
In this study, we found that plasma Trp was significantly increased in the plasma of pigs fed dietary Trp. This could be an indicator for Trp uptake in the small intestine. Similar results were found by Koopmans et al.; they reported that dietary Trp supplementation increased plasma Trp concentration by two times [17]. The result of this study is in accordance with Martínez-Trejo et al. and Li et al. who reported that Trp supplementation affects behavior but did not have any effect on productive performance (FI, DG, and FCR) [18, 19]. The small intestinal histomorphology including villus height, crypt depth, and their ratio is one of important indications of gut health in pigs. A healthy gut has a high villus height to crypt depth ratio. In the present study, pig fed HTS had deeper crypt and lower villus height to crypt depth ratio in the jejunum. These results parallel the findings of Koopmans et al., who suggested that dietary (0.5 g/kg Trp) in nursery pig tends to increase villus height at certain sites along the small intestine [17]. Reduced villus height and increased crypt depth (reduced ratio) lead to increased endogenous secretion and reduced nutrient absorption, disease resistance, and performance [18]. Deep crypts are associated with a high cell turnover. Villi are continually renewed as vulnerable to ordinary sloughing as well as pathogenic assault and pathogen-initiated inflammation [19]. Equally, the high level of activity associated with deeper crypts is costly in energy and nutrients; to obtain adequate nutrients needed for higher mucosal growth may divert energy that is needed for performance. This could be one of the reasons why pig fed HTS had no significant improvement on growth performance in this study.
D-Lactic acid is the final end-product of bacterial fermentation in the gut. Increased plasma D-lactic acid levels reflect changes in intestinal permeability [20]. DAO is an enzyme that serves as an indicator of intestinal epithelial integrity. The intestinal mucosa damaged leads to an increase in serum DAO level [21]. In the present study, HTS increased D-lactate content and DAO activity in the serum of pig fed HTS at d21 after weaning which may indicate impaired intestinal integrity. Tight junction proteins are the principal determinants of epithelial and endothelial paracellular barrier functions [22, 23]. To maintain the integrity of the intestinal barrier, epithelial cells are joined by tight junction proteins, such as claudin, occludin, and ZO-1 [24]. By allowing ions, small molecules, nutrients, and water to cross the cell, whilst restricting pathogens, tight junction proteins mediate the epithelial barrier. The results of this study showed that HTS significantly decreased mRNA expression of tight junction proteins ZO-1 and occludin which was consistent with the increased concentration of serum D-lactate and DAO in the plasma. This suggests that high dietary supplementation of Trp may compromise the intestinal barrier integrity in weaned pig. According to Jiang et al., Trp deficiency or excess could cause antioxidant system disruption and change tight junction protein transcription abundances in the fish gill [25]. One of the most important factors in the growth of intestinal microbiota is gut motility [26]. Intestinal motility, together with mucus secretions, provides another epithelium defense mechanism by forcing pathogens and toxins along the gut lumen to be eventually voided. However, increase in intestinal motility and secretion in the small intestine may lead to intestinal permeability [27]. According to Kojima et al., 5-HT, released from damaged enterochromaffin cells resulting from an allergic reaction, increases the strength and rate of intestinal peristalsis and then contributes to diarrhoea [28]. Overall, our results showed that, at moderate supplementation (0.15%), dietary Trp did not affect pig performance. However, at a much higher level (0.75%), dietary Trp could negatively affect intestinal morphology and tight junction proteins in weaned pigs. The change in morphological and tight junction expression in pig fed high dietary Trp (0.75%) supplementation in the present study provides new information regarding the potentials for using Trp in weaned pigs.
Competing Interests
The authors declare that there are no competing interests regarding the publication of this paper.
Acknowledgments
This study was in part supported by National Natural Science Foundation of China (nos. 31330075, 31110103909, 31501964, 31272463, and 31372326), National Basic Research Program of China (2013CB127302 and 2013CB127301), the Hunan Provincial Natural Science Foundation of China (13JJ2034), National Science and Technology Basic Projects of China (2013FY113300), the Ministry of Agriculture 948 Program (2016-X47 and 2015-Z64), and Technology Innovation Platform for national research institutions located in Hunan province (2013TF3006). This project was also partially financially supported by King Saud University, through Vice Deanship of Research Chairs.