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Oral administration of propionic acid during lactation enhances the colonic barrier function
Lipids in Health and Disease volume 16, Article number: 62 (2017)
Propionic acid is a three-carbon short chain fatty acid (SCFA) that has various effects on colonic functions. Although several studies have shown the effects of propionic acid on intestinal mucosal barrier function, studies of the promotion effect during pre-weaning are rare in the literature as far as we know.
Pre-weaning male Sprague-Dawley rats 7 days after birth were given an oral 0.2 mL/10 g of 200 mM propionic acid solution in the propionic acid group or normal saline solution in the control group by gavage twice a day for ten days. The proximal colonic contents were used for extraction and determination of propionic acid by gas chromatographic analysis; the transepithelial electrical resistance (TER) of colonic tissue was detected by an Ussing chamber; the alterations of ZO-1, Claudin-1, Claudin-8 and Occludin proteins were analyzed by Western blot and immunohistochemistry; and The activity of ERK and p38 MAPK was determined by the phosphorylation status of ERK1/2 and p38 with Western blot.
Our results suggested a higher concentration (23.5 ± 1.9 mmol/kg) of propionic acid compared to the physiological concentration (18.1 ± 0.9 mmol/kg) in colonic contents after oral administration increased the value of TER and the expression of ZO-1, Claudin-1, Claudin-8 and Occludin compared to the control group. Furthermore, the expression levels of phosphorylated ERK1/2 and p38 MAPK were increased in propionic acid group.
We concluded that continuous oral administration of propionic acid during lactation may increase its concentration in the proximal colon and promote epithelial barrier function of proximal colon by enhancing the expression of ZO-1, Claudin-8, Claudin-1 and Occludin via increases in the expression of ERK1/2 and p38 MAPK.
Short chain fatty acids (SCFAs), primarily acetic acid, propionic acid and butyric acid, are mainly produced by the fermentation of fibers and resistant starches that require the presence of specific colonic bacteria . There is now an abundance of evidence to indicate that SCFAs play an important role in the maintenance of health and the development of disease [2, 3]. It has been confirmed that SCFAs can not only serve as the principal energy source for colonic epithelia, but they can also reduce the incidence of colonic inflammatory disease by inhibiting inflammatory cytokine release [4, 5]. In particular, SCFAs are considered to play an important role in anti-tumorigenic activity by inhibiting cancer cell proliferation and inducing apoptosis [6, 7].
The barrier function of colonic mucosa plays a key role in maintaining the balance between host and intestinal microbes. Tight junctions (TJs) as the critical physical intestinal barrier are the principal determinant of mucosal permeability . Occludin, claudins and junctional adhesion molecules are the major transmembrane proteins linked to the cytoskeleton by zonula occludens (ZO), and they constitute the TJ . The intestinal TJ seals the space between adjacent epithelia to effectively prevent pathogenic bacteria, endotoxins and other harmful substances from crossing the mucosa to the blood and the abdominal cavity .
SCFAs can dose-dependently suppress the permeability of isolated colonic mucosa and the Caco-2 cell monolayer in the short term in vitro [11, 12]. However, most of the literature focuses on butyrate and to a lesser extent on acetate. Consequently, the potential effects of propionic acid have long been underestimated . In addition, pre-weaning is a special period in which the intestinal mucosal barrier has not yet matured, which results in the lack of resistance to various stresses . Therefore, the pre-weaning rats were given an oral 2 mL/10 g of 200 mM propionic acid solution by gavage, and our study demonstrated that the oral administration of propionic acid during lactation increased its concentration in the proximal colon and enhanced epithelial barrier function.
Materials and antibodies
Phosphate-buffered saline (PBS) was purchased from Solarbio (Life Sciences Co. Ltd, Beijing, China). acetic acid, propionic acid and butyric acid, ethyl acetate, D-Mannitol, D-(+)-Glucose and agarose were purchased from Sigma (St Louis, MO, USA). Polyclonal rabbit antibodies for ZO-1, Claudin-8, Claudin-1 (Invitrogen Inc., USA), Occludin (Proteintech, Hubei, China), p38 MAPK, phospho-p38 MAPK, ERK1/2, phospho-ERK1/2 (Cell Signaling Technology, USA) and the monoclonal mouse antibody for glyceraldehyde 3-phosphate dehydrogenase (GAPDH) (Bioworld Inc., USA) were used as the primary antibodies. Horseradish peroxidase (HRP)-conjugated goat anti-rabbit IgG antibodies and HRP-conjugated goat anti-mouse IgG antibodies (Bioworld Inc., USA) were used as secondary antibodies. The DAB Detection Kit (Polymer) (ZSGB-BIO, Beijing, China) was used for immunohistochemistry. SuperSignal West Dura Extended Duration Substrate (ThermoFisher, USA) was applied for chemiluminescence.
All of the experimental procedures were performed in compliance with the ethical principles of animal welfare. Pre-weaning male Sprague-Dawley rats (Laboratory Animal Centre, Wenzhou Medical University, China) 7 days after birth (18–20 g) were randomized into the control and propionic acid groups. The rats were given an oral 0.2 mL/10 g of 200 mM propionic acid solution in the propionic acid group or a normal saline solution in the control group by gavage twice a day for ten days. On the 11th experimental day, all of the rats were anesthetized and sacrificed to collect tissue and the contents of the colon.
Gas chromatographic analysis
Each gram of colon contents was thawed and suspended in 5 mL of water and homogenized with a vortex for 2 min, followed by centrifugation (>10,000 r/min) for 10 min. Next, 0.1 mL of 0.5 M sulfuric acid was added to the supernatant of the colon content solution per milliliter to adjust the pH. Each milliliter of supernatant was extracted with 1 mL of ethyl acetate by vortex mixing for 2 min, centrifuged (>10,000 r/min) for 10 min and then incubated at 4 °C for 30 min. The supernatant ethyl acetate extracts were stored at −20 °C before gas chromatography (GC) analysis.
Chromatographic analysis was performed using an Agilent 6890 N GC system equipped with a flame ionization detector (FID) and an N10149 automatic liquid sampler , an HP-INNOWAX column, 30 m × 0.32 mm × 0.25 μm (Agilent, USA), was also used.
The temperature increase procedure was performed as follows: the initial temperature was 100 °C and was maintained for 0.5 min, then increased to 180 °C at 8 °C/min and maintained for 1 min, then increased to 200 °C at 20 °C/min, and finally maintained at 200 °C for 5 min. The temperatures of the injection port and FID detector were 200 °C and 240 °C, respectively. The flow rate of nitrogen was 20 mL/min with a split ratio of 1:10. 1 μL sample solution was injected for analysis. The SCFAs were identified by their specific retention times under the above GC conditions. Propionic acid calibration curve was made in the range of 0.75–6 mmol/L, and the concentration of the sample solution was converted to the propionic acid concentration in the colon contents.
Transepithelial electrical resistance (TER) in the colonic wall using an Ussing chamber
Approximately 2 cm of colonic tissues were quickly taken from the rats within 5 min after anesthetization. Each specimen was opened along the mesenteric line and then rinsed with ice-cold 0.9% sodium chloride solution and kept in the same solution aerated with carbogen (95% O2–5% CO2) before being mounted in an Ussing chamber. Prepared colonic specimens were mounted on a 6-Channel EasyMount Ussing Chamber System (Physiologic Instruments, USA) that exposed a circular area of 0.031 cm2. Then, 5 mL of Manital-Krebs buffer was added to the side of the mucosa while 5 mL of Glucose-Krebs buffer was added to the serosa side. The Ussing chamber system was maintained at a constant temperature of 37 °C by using circulating water, and the medium on both sides was filled with carbogen (95% O2–5% CO2). Transepithelium electrical resistance (TER) was recorded for each specimen for 120 min after a 10 min stable period using the Ussing chamber technique.
After being excised and rinsed with ice-cold 0.9% sodium chloride solution, the proximal colons were homogenized by mechanical disruption in lysis buffer (50 mM Tris pH 7.4, 150 mM NaCl, 1% TritonX-100, 1% sodium deoxycholate, 0.1% SDS, 2 mM sodium pyrophosphate, 25 mM β-glycerophosphate, 1 mM EDTA, 1 mM Na3VO4, 0.5 mg/L leupeptin, 1 mM PMSF) and incubated on ice for 30 min. The lysates were centrifuged (10,000 r/min) for 30 min. The protein extracts were used to determine the quantity of total protein with the BCA method, and the extracts were boiled with SDS loading buffer and separated by 10% SDS–PAGE gels. After transferring the proteins to polyvinylidene fluoride membranes, the blotting procedure was performed as follows: the membranes were blocked in 5% nonfat milk in Tris Buffered Saline with Tween-20 detergent (TBST) for two hours at room temperature, incubated with primary antibodies (rabbit anti-Claudin-1, Claudin-8, Occludin, p38 MAPK, phospho-p38 MAPK, ERK1/2, phospho-ERK1/2, 1:1000 and mouse anti-GAPDH, 1:5000) overnight at 4 °C and then incubated with secondary antibodies for two hours at room temperature. The chemiluminescent signals of the bands were collected using the ChemiDoc MP system (Bio-Rad, USA). Quantification of protein intensity was performed using Image J software, and the results were expressed as the ratio of relative intensity of target proteins to the internal standard, GAPDH.
Next, 4 μm sections were placed on clean, positively-charged microscope slides and heated in a tissue-drying oven for 2 h at 60 °C. The sections were washed in xylene 3 times for 5 min for deparaffinization and hydrated through a series of graded concentrations of alcohol. The slides were heated in 10 mM sodium citrate buffer at pH 6.0 at 100 °C for 20 min and cooled by incubation at room temperature in buffer for 20 min for antigen retrieval. Endogenous peroxidase activity was blocked with 3% H2O2 for 5 min. Subsequently, sections were blocked with BSA for 30 min and then incubated with the primary antibodies (rabbit anti-ZO-1, Claudin-8, 1:300) overnight at 4 °C. Afterwards, the sections were incubated with the biotinylated goat anti-rabbit IgG polymer for 20 min at room temperature. Immunoreactivity was visualized by diaminobenzidine, and the sections were counterstained with hematoxylin. Finally, the slides were dehydrated and mounted. A microscope (BX51, OLYMPUS, Japan) was used to examine the specimens.
Statistical analyses were conducted using SPSS Statistics 23.0 (IBM Corporation, USA) and Prism 7.0 (GraphPad Software, Inc. USA) for Mac OS X. All of the data are shown as the means ± standard deviation (SD). Data on the TER were analyzed using a repeated measures analysis of variance (ANOVA), and the t test was used for the comparison between the two groups. P < 0.05 referred to significant differences.
Administration of propionic acid by oral gavage enhanced the concentration in colonic contents
Figure 1a shows a typical chromatogram of a standard mixture containing the major SCFAs (acetic acid, propionic acid and butyric acid). The standard mixture was dissolved in ethyl acetate, and the peaks were identified by comparing retention times after injecting a series of graded concentrations of the individual SCFAs. To measure the concentration of propionic acid in the colonic contents, the calibration curve of propionic acid (y = 3.8431 × + 16.915, where (x) is the concentration (mM) and (y) is the peak area count) was performed and showed good linearity (R2 ≥ 0.997) for a wide range of concentrations (4–32 mM) that allowed the measurement of propionic acid in the proximal colon content samples. Figure 1b, d shows a chromatogram of SCFAs, particularly propionic acid in the colonic content samples of the control group and the propionic acid group. The difference of the concentration of propionic acid in the colonic contents between the oral administration of the normal saline solution and propionic acid by gavage is shown in Fig. 1c. The concentration of propionic acid in the control group (18.1 ± 0.9 mmol/kg) and the propionic acid group (23.5 ± 1.9 mmol/kg) was measured by the GC method, as previously described, and both concentrations were in the range of the physiological concentration in the proximal colon. The propionic acid content in the proximal colon after the rats were given an oral 2 mL/10 g of 200 mM propionic acid solution by gavage twice a day was significantly higher than the control group (P < 0.05).
Higher concentration of propionic acid enhanced intestinal epithelial barrier function
TER was detected by the Ussing chamber system, which is a representation of intestinal epithelial barrier function , and a trend of slowing down for both the control and propionic acid groups over the 120 min incubation time in vitro was found. However, the TER was significantly higher after the rats received 200 mM propionic acid by oral gavage twice a day for ten days compared to treatment with normal saline solution at all time points, particularly the initial value at 0 min (propionic acid group: 86.2 ± 11.6 Ω.cm2, control group: 69.4 ± 10.5 Ω.cm2), as shown in Fig. 2 (P < 0.05).
A higher concentration of propionic acid enhanced the intestinal barrier by increasing the expression of Claudin-1, Claudin-8 and Occludin
Transmembrane elements, such as occludin and claudin, as well as the peripheral membrane protein ZO-1, are major components of the TJ. A ~22 kDa band for Claudin-1, ~30 kDa for Claudin-8 and ~59 kDa for Occludin appeared in the Western blot analyses and demonstrated changes in expression after the oral administration of 200 mM propionic acid compared to the control group. Figure 3a shows the signal bands of proteins detected at the expected molecular weights. The results of the proteins expression were summarized as a ratio of relative intensity of the target proteins to GAPDH, as shown in Fig. 3b, c, d. The expression of Claudin-1, Claudin-8 and Occludin in the proximal colon increased significantly compared to the control group (P < 0.05).
ZO-1 and Occludin staining in proximal colon epithelia
Immunohistochemistry was performed to analyze the expression and distribution of TJs in the proximal colon by staining for the ZO-1 and Claudin-8 proteins. As Fig. 4 shows, ZO-1 and Claudin-8 were located at the superficial layer of the colonal mucosa connecting the epithelia and were consistent with TJ distribution. The staining intensity of ZO-1 and Claudin-8 in the propionic acid group (Fig. 4c, d) was significantly higher for both proteins compared to the control group (Fig. 4a, b) (P < 0.05), which agreed with the results of the Western blots. In addition, the enhancement of Claudin-8 expression was more obvious compared to that of ZO-1.
Propionic acid enhanced the intestinal barrier via phosphorylation of ERK1/2 and p38 MAPK
We measured the changes in phosphorylation status of ERK1/2 (~44/42KD) and p38 (~43KD) after the oral administration of 200 mM propionic acid. Figure 5a, b shows the signal bands of proteins detected at the expected molecular weights and the expression levels of phosphorylated ERK1/2, p38 MAPK were significantly increased in the propionic acid group compared to the control group (P < 0.05).
During lactation, individuals are susceptible to intestinal diseases, such as necrotizing enterocolitis, because the intestinal mucosal barrier has not yet matured and there is a lack of resistance to various stressors . Therefore, pre-weaning male Sprague-Dawley rats 7 days after birth, which simulated the neonatal period in humans, were used as models in our research. Their proximal colonic contents were extracted, and we determined the amount of propionic acid in the contents after the continuous oral administration of 200 mM propionic acid for ten days. The results of the GC analysis revealed that the propionic acid group had a greater propionic acid concentration in the proximal colon compared to the control group. Therefore, we discovered that the oral administration of 0.2 mL/10 g of 200 mM propionic acid by gavage increased the propionic acid concentration even though a majority of the propionic acid was absorbed by the small intestine .
In the physical environment, the primary amount of propionic acid was derived from the fermentation of undigested food by the colonic microbiota. Propionic acid has various functions in the colon as a major player in the maintenance of gut and immune homeostasis [19, 20]. The physiological concentration of propionic acid could immediately enhance barrier function of the colonic epithelium over a short period of time in vitro [21, 22]. As far as we know, studies of the long-term promotion effect of propionic acid in the colon in vivo, particularly for pre-weaning rats, are limited. To maintain the intact structure of the proximal colon epithelium , we detected the TER of whole colonic tissues with an Ussing chamber. The results showed that a higher concentration of propionic acid could promote proximal colonic barrier function in vivo, which was supported by greater TER values. The TJ is the most important structure in the mucosal barrier, and it plays a critical role in the maintenance of mucosal barrier function . We assumed that a higher concentration of propionic acid may influence the expression of ZO-1, Claudin-8, Claudin-1 and Occludin, which are the major components of the TJ. The results of the Western blots demonstrated that the expression levels of Claudin-1, Claudin-8 and Occludin increased after the oral administration of 200 mM propionic acid for ten days; moreover, the immunohistochemistry of ZO-1 and Claudin-8 was consistent with the Western blot results.
Numerous studies have shown that under pathological conditions, such as inflammatory bowel disease and obesity, the increase in gut permeability is associated with much lower concentrations of SCFAs in the intestine [2, 24]. Oral supplementation of SCFAs after intestinal damage can suppress colonic epithelial permeability [25–27]. Furthermore, under physiologic status, the long-term promotive effect of a higher concentration of propionic acid on proximal colonic barrier function of pre-weaning rats was confirmed in our study.
Several molecular mechanisms by which SCFAs to modulate biological responses of the host have been proposed and elucidated. The major mechanisms involves the direct inhibition of histone deacetylases (HDACs) to directly regulate gene expression [28–30] and signaling through G-protein-coupled receptors (GPCRs) [31–33]. Propionic acid was the most potent and efficacious ligand for GPCR4 . In this study, we showed that phosphorylated ERK1/2 and p38 MAPK were more strongly expressed in colonal mucosa after the oral administration of 200 mM propionic acid during lactation compared to the control group. As an intracellular mechanism, the ERK1/2 or p38 MAPK pathways is acknowledged as one of signals downstream of GPCRs [35–37]. It was previously reported that the ERK1/2 and p38 pathways are involved in the regulation of cell proliferation . Therefore, our study suggested that ERK1/2 and p38 MAPK signaling pathways were involved in the propionic acid related promotion effect on colonic barrier function. But, the mechanism underlying the propionic acid activation of ERK1/2 and p38 MAPK remains to be further elucidated.
We concluded that continuous oral administration of propionic acid during lactation may increase its concentration in the proximal colon and promote epithelial barrier function of proximal colon by enhancing the expression of ZO-1, Claudin-8, Claudin-1 and Occludin via increases in the expression of ERK1/2 and p38 MAPK. Our results also highlighted the potential value of propionic acid for the prevention and treatment of intestinal diseases, such as necrotizing enterocolitis, and the regulation of nutrition in newborns.
Glyceraldehyde 3-phosphate dehydrogenase
Short chain fatty acid
Transepithelial electrical resistance
Rios-Covian D, Ruas-Madiedo P, Margolles A, Gueimonde M, de Los Reyes-Gavilan CG, Salazar N. Intestinal short chain fatty acids and their link with diet and human health. Front Microbiol. 2016;7:185.
Tan J, McKenzie C, Potamitis M, Thorburn AN, Mackay CR, Macia L. The role of short-chain fatty acids in health and disease. Adv Immunol. 2014;121:91–119.
Kasubuchi M, Hasegawa S, Hiramatsu T, Ichimura A, Kimura I. Dietary gut microbial metabolites, short-chain fatty acids, and host metabolic regulation. Nutrients. 2015;7:2839–49.
Clausen MR, Mortensen PB. Kinetic studies on colonocyte metabolism of short chain fatty acids and glucose in ulcerative colitis. Gut. 1995;37(5):684–9.
Vinolo MA, Rodrigues HG, Hatanaka E, Sato FT, Sampaio SC, Curi R. Suppressive effect of short-chain fatty acids on production of proinflammatory mediators by neutrophils. J Nutr Biochem. 2011;22:849–55.
Kolar SS, Barhoumi R, Lupton JR, Chapkin RS. Docosahexaenoic acid and butyrate synergistically induce colonocyte apoptosis by enhancing mitochondrial Ca2+ accumulation. Cancer Res. 2007;67:5561–8.
Borthakur A, Priyamvada S, Kumar A, Natarajan AA, Gill RK, Alrefai WA, Dudeja PK. A novel nutrient sensing mechanism underlies substrate-induced regulation of monocarboxylate transporter-1. Am J Physiol Gastrointest Liver Physiol. 2012;303:G1126–33.
Turner JR. Intestinal mucosal barrier function in health and disease. Nat Rev Immunol. 2009;9:799–809.
Blaskewicz CD, Pudney J, Anderson DJ. Structure and function of intercellular junctions in human cervical and vaginal mucosal epithelia. Biol Reprod. 2011;85:97–104.
Kondoh M, Takahashi A, Yagi K. Spiral progression in the development of absorption enhancers based on the biology of tight junctions. Adv Drug Deliv Rev. 2012;64:515–22.
Valenzano MC, DiGuilio K, Mercado J, Teter M, To J, Ferraro B, Mixson B, Manley I, Baker V, Moore BA, Wertheimer J, Mullin JM. Remodeling of tight junctions and enhancement of barrier integrity of the CACO-2 intestinal epithelial cell layer by micronutrients. PLoS One. 2015;10:e0133926.
Reimer RA, Maathuis AJ, Venema K, Lyon MR, Gahler RJ, Wood S. Effect of the novel polysaccharide PolyGlycopleX(R) on short-chain fatty acid production in a computer-controlled in vitro model of the human large intestine. Nutrients. 2014;6:1115–27.
Al-Lahham SH, Peppelenbosch MP, Roelofsen H, Vonk RJ, Venema K. Biological effects of propionic acid in humans; metabolism, potential applications and underlying mechanisms. Biochim Biophys Acta. 2010;1801(11):1175–83.
Steele MA, Penner GB, Chaucheyras-Durand F, le Guan L. Development and physiology of the rumen and the lower gut: targets for improving gut health. J Dairy Sci. 2016;99:4955–66.
Zhao G, Nyman M, Jonsson JA. Rapid determination of short-chain fatty acids in colonic contents and faeces of humans and rats by acidified water-extraction and direct-injection gas chromatography. Biomed Chromatogr. 2006;20:674–82.
Wong JM, de Souza R, Kendall CW, Emam A, Jenkins DJ. Colonic health: fermentation and short chain fatty acids. J Clin Gastroenterol. 2006;40(3):235–43.
Clarke LL. A guide to Ussing chamber studies of mouse intestine. Am J Physiol Gastrointest Liver Physiol. 2009;296(6):G1151–66.
Kaji I, Iwanaga T, Watanabe M, Guth PH, Engel E, Kaunitz JD, Akiba Y. SCFA transport in rat duodenum. Am J Physiol Gastrointest Liver Physiol. 2015;308:G188–97.
Al-Lahham S, Roelofsen H, Rezaee F, Weening D, Hoek A, Vonk R, Venema K. Propionic acid affects immune status and metabolism in adipose tissue from overweight subjects. Eur J Clin Invest. 2012;42:357–64.
Tong LC, Wang Y, Wang ZB, Liu WY, Sun S, Li L, Su DF, Zhang LC. Propionate ameliorates dextran sodium sulfate-induced colitis by improving intestinal barrier function and reducing inflammation and oxidative stress. Front Pharmacol. 2016;7:253.
Suzuki T, Yoshida S, Hara H. Physiological concentrations of short-chain fatty acids immediately suppress colonic epithelial permeability. Br J Nutr. 2008;100:297–305.
Kelly CJ, Zheng L, Campbell EL, Saeedi B, Scholz CC, Bayless AJ, Wilson KE, Glover LE, Kominsky DJ, Magnuson A, Weir TL, Ehrentraut SF, Pickel C, Kuhn KA, Lanis JM, Nguyen V, Taylor CT, Colgan SP. Crosstalk between microbiota-derived short-chain fatty acids and intestinal epithelial HIF augments tissue barrier function. Cell Host Microbe. 2015;17(5):662–71.
Li C, Li Q, Liu YY, Wang MX, Pan CS, Yan L, Chen YY, Fan JY, Han JY. Protective effects of Notoginsenoside R1 on intestinal ischemia-reperfusion injury in rats. Am J Physiol Gastrointest Liver Physiol. 2014;306:G111–22.
Voltolini C, Battersby S, Etherington SL, Petraglia F, Norman JE, Jabbour HN. A novel antiinflammatory role for the short-chain fatty acids in human labor. Endocrinology. 2012;153:395–403.
Vieira ELM, Leonel AJ, Sad AP, Beltrão NRM, Costa TF, Ferreira TMR, Gomes-Santos AC, Faria AMC, Peluzio MCG, Cara DC, Alvarez-Leite JI. Oral administration of sodium butyrate attenuates inflammation and mucosal lesion in experimental acute ulcerative colitis. J Nutr Biochem. 2012;23:430–6.
Ferreira TM, Leonel AJ, Melo MA, Santos RR, Cara DC, Cardoso VN, Correia MI, Alvarez-Leite JI. Oral supplementation of butyrate reduces mucositis and intestinal permeability associated with 5-Fluorouracil administration. Lipids. 2012;47:669–78.
Ramos MG, Bambirra EA, Cara DC, Vieira EC, Alvarez‐Leite JI. Oral administration of short‐chain fatty acids reduces the intestinal mucositis caused by treatment with Ara‐C in mice fed commercial or elemental diets. Nutr Cancer. 1997;28:212–7.
Han A, Bennett N, MacDonald A, Johnstone M, Whelan J, Donohoe DR. Cellular metabolism and dose reveal carnitine-dependent and -independent mechanisms of butyrate oxidation in colorectal cancer cells. Cell Physiol. 2016;231:1804–13.
Zapletal O, Tylichova Z, Neca J, Kohoutek J, Machala M, Milcova A, Pokorna M, Topinka J, Moyer MP, Hofmanova J, Kozubik A, Vondracek J. Butyrate alters expression of cytochrome P450 1A1 and metabolism of benzo pyrene via its histone deacetylase activity in colon epithelial cell models. Arch Toxicol. 2016. doi:10.1007/s00204-016-1887-4.
Schilderink R, Verseijden C, Seppen J, Muncan V, van den Brink GR, Lambers TT, van Tol EA, de Jonge WJ. The SCFA butyrate stimulates the epithelial production of retinoic acid via inhibition of epithelial HDAC. Am J Physiol Gastrointest Liver Physiol. 2016;310:G1138–46.
Yajima T, Inoue R, Yajima M, Tsuruta T, Karaki S, Hira T, Kuwahara A. The G-protein on cholesterol-rich membrane microdomains mediates mucosal sensing of short- chain fatty acid and secretory response in rat colon. Acta Physiol (Oxf). 2011;203:381–9.
Zaiss MM, Rapin A, Lebon L, Dubey LK, Mosconi I, Sarter K, Piersigilli A, Menin L, Walker AW, Rougemont J, Paerewijck O, Geldhof P, McCoy KD, Macpherson AJ, Croese J, Giacomin PR, Loukas A, Junt T, Marsland BJ, Harris NL. The intestinal microbiota contributes to the ability of helminths to modulate allergic inflammation. Immunity. 2015;43:998–1010.
Kim MH, Kang SG, Park JH, Yanagisawa M, Kim CH. Short-chain fatty acids activate GPR41 and GPR43 on intestinal epithelial cells to promote inflammatory responses in mice. Gastroenterology. 2013;145:396–406.
Le Poul E, Loison C, Struyf S, Springael JY, Lannoy V, Decobecq ME, Brezillon S, Dupriez V, Vassart G, Van Damme J, Parmentier M, Detheux M. Functional characterization of human receptors for short chain fatty acids and their role in polymorphonuclear cell activation. Biol Chem. 2003;278:25481–9.
Miyamoto J, Mizukure T, Park SB, Kishino S, Kimura I, Hirano K, Bergamo P, Rossi M, Suzuki T, Arita M, Ogawa J, Tanabe S. A gut microbial metabolite of linoleic acid, 10-hydroxy-cis-12-octadecenoic acid, ameliorates intestinal epithelial barrier impairment partially via GPR40-MEK-ERK pathway. Biol Chem. 2015;290:2902–18.
Owens DM, Keyse SM. Differential regulation of MAP kinase signalling by dual-specificity protein phosphatases. Oncogene. 2007;26:3203–13.
Hofmann NA, Yang J, Trauger SA, Nakayama H, Huang L, Strunk D, Moses MA, Klagsbrun M, Bischoff J, Graier WF. The GPR 55 agonist, L-alpha-lysophosphatidylinositol, mediates ovarian carcinoma cell-induced angiogenesis. Br J Pharmacol. 2015;172:4107–18.
Zeng Z, Leng T, Feng X, Sun H, Inoue K, Zhu L, Xiong ZG. Silencing TRPM7 in mouse cortical astrocytes impairs cell proliferation and migration via ERK and JNK signaling pathways. PLoS One. 2015;10:e0119912.
This work was supported by natural science foundation of Zhejiang Province (Y13H040029), and public welfare science and technology project of Wenzhou (Y20150021).
Availability of data and materials
The datasets used during the current study available from the corresponding author on reasonable request.
Design of the study: ZR L, LB Z; conduct of the study: ZB X, YJ H, K W, SK G, XZ H, ZR L; data collection: ZB X, K W; data analysis: ZB X, SK G; manuscript writing: ZB X; all authors read and approved the final manuscript.
The authors declare that they have no competing interests.
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All procedures were approved by the Ethics Committee for Use of Experimental Animals at the Wenzhou Medical University (Zhejiang, China).
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Xia, Z., Han, Y., Wang, K. et al. Oral administration of propionic acid during lactation enhances the colonic barrier function. Lipids Health Dis 16, 62 (2017). https://doi.org/10.1186/s12944-017-0452-3
- Propionic acid
- Barrier function
- Tight junction
- Ussing chamber
- Gas chromatography