- Research article
- Open Access
Severe burn injury alters intestinal microbiota composition and impairs intestinal barrier in mice
Burns & Trauma volume 7, Article number: 20 (2019)
The intestinal barrier integrity is crucial for maintaining intestinal homeostasis, and the mechanisms of intestinal barrier disruption induced by burn injury remain obscure. This study was aimed to investigate the changes of intestinal microbiota and barrier function in burned mice to further comprehend the mechanisms of burn-induced intestinal barrier dysfunction.
Samples were from mice inflicted with 30% total body surface area (TBSA) full-thickness burns. The intestinal permeability, tight junction proteins expressions, zonula occludens-1 (ZO-1) localization, inflammatory cytokines expressions, and short-chain fatty acids (SCFAs) contents were determined. The microbial community was assessed via 16S rDNA Illumina sequencing.
The intestinal permeability was increased after severe burn injury, peaking at 6 h post-burn, with approximately 20-folds of the control (p < 0.001). The expression of tight junction proteins (ZO-1, occludin, claudin-1, and claudin-2) was significantly altered (p < 0.05). The ZO-1 morphology was dramatically changed following burn injury. The fecal SCFAs’ contents (acetate, propionate, butyrate, isobutyrate, and isovalerate) were noticeably declined after burn injury (p < 0.05). The expressions of pro-inflammatory cytokines (interleukin (IL)-1β and IL-6) in ileal mucosa were increased, whereas the expressions of anti-inflammatory cytokines (IL-4 and IL-13) were decreased following burn injury (p < 0.05). In addition, burned mice showed an alteration of intestinal microbial community, such as decreased diversity, reduced Bacteroidetes abundance, and increased Firmicutes abundance.
The severe burn-induced intestinal barrier dysfunction is along with the alterations of microbial community.
The intestinal epithelial barrier integrity plays a crucial role in preventing pathogens and other molecules from entering the intestinal mucosa and interacting with the immune system, in which tight junction are principal structural factors [1,2,3,4]. However, the intestinal barrier is destroyed in some severe surgical diseases, such as trauma, shock, and burn injury, resulting in augmented intestinal permeability and subsequent bacterial translocation or/and endotoxin. The disrupted intestinal epithelial barrier is responsible for systemic inflammatory response syndrome, sepsis, multiple organ dysfunction syndrome, and other severe complications [5,6,7]. Thus, further investigating the mechanisms of intestinal barrier disruption and developing corresponding therapeutic strategies to maintain intestinal barrier are meaningful.
Virtually, human individuals live in close association with surrounding microbes, especially the microorganisms inhabiting in the gastrointestinal tract. The microorganisms residing in the gastrointestinal tract are referred as the gut microbiota , which is important for host physiological and pathological processes such as intestinal epithelial barrier reinforcement, immune system development, and nutrients absorption . It has been demonstrated that intestinal ischemia/reperfusion, which often occurs at the early stage of severe burn injury, induce the dysbiosis of gut microbiota . However, the detailed alteration of intestinal microbiota composition in severe burn injury still needs to be clarified.
Short-chain fatty acids (SCFAs), including acetate, propionate, butyrate, isobutyrate, and isovalerate, are bacterial metabolites generated through fermentating dietary fibers. Luminal SCFAs, which are recognized as preferred energy substrates for colonic epithelia, influence epithelial barrier function, mucosal immune systems, and inflammatory responses , for example, butyrate for colitis by promoting regulatory T cells’ (Tregs) formation, decreasing pro-inflammatory cytokines, activating Gpr109a to suppress inflammatory signals, and enhancing intestinal barrier [12,13,14,15,16,17]. It has been documented that gut microbiota deficiency is associated with increased blood-brain barrier permeability, which may be attributed to altered SCFAs . Even so, the role of SCFAs on intestinal barrier remains obscure.
In this study, we report that severe burn injury could disrupt intestinal microbiota community, alter inflammatory cytokines, decrease luminal SCFAs, and disrupt intestinal epithelial barrier. Thus, it is suggested that intestinal microbiota dysbiosis may contribute to the barrier dysfunction following a severe burn.
Healthy adult female C57BL/6 mice weighing 18–22 g were used in this study. All the mice were supplied by the Animal Institutes of Daping Hospital, the Third Military Medical University (Army Medical University). The animals were housed in wire-bottomed and wire-lid cages, allowed access to chow and water ad libitum, and acclimatized for 1 week before experiments in a temperature-controlled room (25 ± 2 °C) with 12-h light and dark cycles. The animal studies were approved by the Animal Care and Use Committee of Third Military Medical University (Army Medical University), and all the protocols were approved by the Medical and Ethics Committee of Southwest Hospital, Third Military Medical University (Army Medical University), Chongqing, China.
Burn model and experimental protocol
The burn model was created according to the method usually used in our laboratory . In brief, the control group and burn group received the same treatment expect the scald burn. At the end of the experiment, the mice were anesthetized to detect intestinal permeability and collect intestinal tissue and fecal samples. The control mice were sacrificed immediately after sham burn treatment (0 h), but not at each time point. The harvested tissues and feces were respectively used for immunofluorescent assay, immunoblot, liquid chip, headspace gas chromatography-mass spectrometry (HS-GC/MS), DNA isolation, and microbiota community analysis, as described below.
In vivo intestinal paracellular permeability assay
In this part, we applied the methods which described in previous articles . In brief, after the mice were anesthetized, a 5-cm segment of ileum was dissociated, and then, 0.1 ml of 20 mg/ml fluorescein isothiocyanate-labeled (FITC)-dextran was injected in this segment. After 30 min, the blood sample was collected for fluorescence intensity detection by using a microplate reader (Varioskan Flash, Thermo Electron Corporation, Vantaa, Finland) with wavelength of 480 nm/520 nm. And then, the intestinal permeability was calculated according to the standard curve.
Immunofluorescent staining, microscopy, and image analysis.
We applied the methods which usually utilized and described in previous articles . Frozen sections of ileum were prepared for detecting ZO-1 morphology. After preparatory work, the sections were incubated with monoclonal rabbit antibody against zonula occludens (ZO)-1 (Invitrogen, Carlsbad, CA) diluted at 1:200 in 5% normal goat serum in phosphate buffer saline (PBS) at 4 °C overnight. Then the sections were incubated with secondary Alexa Fluor 488-conjugated goat anti-rabbit IgG antibody (Invitrogen) at 1:200, Alexa Fluor 594-conjugated phalloidin (Invitrogen) at 1:100, and diamidine-2-penylindole (DAPI) (Sigma) at 1:1000 for 1 h at room temperature. Images were obtained using a TCS SP5 laser confocal microscopy (Leica, Germany).
Immunoblot analysis of tight junction proteins
In this part, we applied the methods described in previous articles . In brief, the total tissue proteins were collected for the determination of ZO-1, occludin, claudin-1, and claudin-2. By the way, equal amounts of total protein extracted from the ileal mucosa were respectively fractionated on 8%, 10%, and 12% sodium dodecyl sulfate- polyacrylamide gel electrophoresis (SDS-PAGE) gel and then transferred to polyvinylidene difluoride (PDVF) membrane (Millipore, Bedford, MA). Furthermore, after the membrane was blocked, the membranes were incubated with antibodies specific for ZO-1 (1:1000, Invitrogen), occludin (1:1000, Invitrogen), claudin-1 (1:1000, Invitrogen), claudin-2 (1:1000, Abcam), and β-actin (1:5000, Sigma) overnight at 4 °C. After washing with Tris-buffered saline Tween-20 (TBST), membranes were incubated with appropriate peroxidase-conjugated secondary antibodies (KPL, America) at room temperature for 60 min. The chemiluminescence signal was captured using a ChemiDox XRS system (Bio-Rad). The densities of the bands were quantified with Quantity One Image software (Bio-Rad).
Fecal SCFAs analysis via HS-GC/MS
Fresh ileocecal fecal matters were frozen immediately and stored at − 80 °C until processing. The weighed fecal matters were put into a 20 ml headspace sampling bottle, followed by the addition of 0.95 ml 6% H3PO4 and 0.05 ml 2.49 mmol/l of 2-ethylbutyric acid (the internal standard, diluted by 6% H3PO4), and vibration for 1 min. Then, the samples were injected into the GC/MS system (5975A/7890C Agilent) for analysis. Ultrapure Helium (1.0 ml/min) was used as the carrier gas. Headspace was maintained at 80 °C with incubation time of 30 min. The gas chromatography (DB-FFAP fused-silica capillary column: 30 m × 0.25 mm × 0.25 μm Agilent) stepwise thermal conditions were as follows: 50 °C for 1 min, 10 °C/min until 250 °C for 2 min; the injector temperature was 250 °C, with split ratio of 5: 1. The mass detector system was operated in electron impact ionization at 70 eV, set to scan mode for m/z 33–200, and in single ion monitoring (SIM) mode. The temperatures of the transfer line (interface) and source were maintained at 280 °C and 250 °C, respectively. The monitored ions were m/z 60 and 43.1 for acetic acid, m/z 74.1 and 28.1 for propionic acid, m/z 60 and 73.1 for butyric acid, m/z 60 and 87.1 for isovaleric acid, m/z 43.1 and 73.1 for isobutyric acid, and m/z 88.1 and 73.1 for 2-ethylbutyric. Data acquisition and analysis were done with Saturn GC/MS workstation software (Agilent).
Microbial diversity analysis
Fresh ileocecal fecal matters were collected and frozen immediately at − 80 °C for DNA extraction. Microbial DNA was extracted with the QIAamp® Fast DNA Stool Mini Kit (Qiagen, Valencia, CA) according to the manufacturer’s protocols and then stored at − 80 °C.
Polymerase chain reaction (PCR) amplification
The V3-V4 region of bacterial 16S rDNA gene was amplified using primers 338F (5′-ACTCCTACGGGAGGCAGCAG-3′) and 806R (5′-GGACTACHVGGGTWTCTAAT-3′). The PCR reactions (95 °C for 3 min, followed by 27 cycles at 95 °C for 30 s, 55 °C for 30 s, and 72 °C for 45 s and a final extension at 72 °C for 10 min) were performed in 20-μl mixture containing 4 μl of 5× FastPfu Buffer, 2 μl of 2.5 mmol/l dNTPs, 0.8 μl of primers (5 μmol/l), 0.4 μl of FastPfu Polymerase, and 10 ng of template DNA. Illumina MiSeq sequencing amplicons were extracted from 2% agarose gels, purified using the AxyPrep DNA Gel Extraction Kit (Axygen Biosciences, Union City, CA, USA) according to the manufacturer’s instructions, and quantified using QuantiFluor™-ST (Promega, USA). The purified amplicons were pooled in equimolar and paired-end sequenced (2 × 250) on an Illumina MiSeq platform according to the standard protocols. The raw reads were deposited into the NCBI Sequence Read Archive (SRA) database.
Processing of sequencing data
The raw fastq files were demultiplexed, quality-filtered using QIIME (version 1.9.1) with the following criteria: (i) the 300 bp reads were truncated at any site receiving an average quality score < 20 over a 50 bp sliding window, discarding the truncated reads that were shorter than 50 bp; (ii) exact barcode matching, 2 nucleotide mismatch in primer matching, reads containing ambiguous characters were removed; (iii) and only sequences that overlap longer than 10 bp were assembled according to their overlap sequence. The reads which could not be assembled were discarded. Operational taxonomic units (OTUs) were clustered with 97% similarity cutoff using UPARSE (version 7.1 http://drive5.com/uparse/), and chimeric sequences were identified and removed using UCHIME. The taxonomy of each 16S rRNA gene sequence was analyzed by RDP Classifier (http://rdp.cme.msu.edu/) against the silva (SSU123)16S rRNA database using confidence threshold of 70% .
Inflammatory cytokines analysis by liquid chip
After the animals were sacrificed, an appropriate ileal segment was taken to harvest mucosa by a glass slide. The harvested mucosa was homogenized in ice-cold PBS containing protease inhibitor cocktails (Millipore), followed by a brief sonication with a sonicator (Tomy Seiko, Tokyo, Japan), and a centrifugation at 12000 rpm, 4 °C for 15 min. The supernatants were collected for the determination of inflammatory cytokines by Merck Millipore Liquid Chip Kit (Millipore) according to the manufacturer’s protocols.
Data are presented as means ± standard error of the mean (SEM). For data analysis, Dunnett’s t test was performed against the control group only using SPSS 13.0 statistical software. A p value of < 0.05 was considered as minimum level of significance in all cases. All reported significance levels represent two-tailed p values.
Severe burn increased intestinal permeability
We analyzed the intestinal barrier permeability in mice (sham or 30% total body surface area (TBSA) full-thickness burn) through measuring the concentration in plasma of 4.4 kDa FITC-dextran, which is traditionally used in this experiment. As shown in Fig. 1, when compared with control (0 h), the FITC-dextran concentration started to increase significantly at 1 h after burn, peaked at 6 h with approximately 20-folds of control, and was still significantly higher than that of control on 1, 3, 5, and 7 days after burn injury. These results indicate that the intestinal paracellular permeability is significantly increased in burned mice, suggesting that severe burn injury can destroy intestinal epithelial barrier.
Severe burn changed tight junction proteins’ expressions
To more precisely understand the intestinal barrier dysfunction induced by burn injury, we next evaluated the expressions of ZO-1, occludin, claudin-1, and claudin-2, which are important members of tight junction proteins. As illustrated in Fig. 2a–c, when compared with control, the expressions of ZO-1, occludin, and claudin-1 decreased significantly after burn injury. Both ZO-1 and claudin-1 reduced to the minimum on 1 day post-burn, whereas occludin dropped to the lowest level at 6 h post-burn. In addition, ZO-1 expression gradually increased after 1 day and almost increased to the control level on 7 days post-burn. The expressions of both occludin and claudin-1 following burn injury were always lower than those of control. On the contrary, as shown in Fig. 2d, claudin-2, a pore-forming protein , was remarkably increased at all time points after burn injury, peaking at 6 h post-burn. These results indicate that the expressions of tight junction proteins are significantly changed after severe burn injury, which may result in the disruption of intestinal barrier.
Severe burn disrupted ZO-1 morphology
To more comprehensively illuminate severe burn-induced intestinal barrier deficiency, we assessed the alterations of ZO-1 morphology by immunofluorescent. As shown in Fig. 3, in control mice, ZO-1 was distributed to the epithelial tight junction, which was appreciated as red spots and almost a straight line, lying at the apical compartment of cell-cell junctions. In contrast, the ordered ZO-1 morphology was disrupted in the ileum of burned mice, especially at 6 h post-burn. These morphological alterations of ZO-1 were consistent with the abovementioned changes of intestinal permeability after burn injury. Thus, severe burn injury could alter ZO-1 morphology, contributing to the intestinal barrier dysfunction.
Severe burn changed inflammatory cytokines’ expressions
To determine the involvements of inflammatory cytokines in the burn-induced intestinal barrier dysfunction, we analyzed the expressions of interleukin (IL)-1β, IL-6, IL-4, IL-10, and IL-13 in ileal mucosa. As shown in Fig. 4, the contents of pro-inflammatory cytokines IL-1β and IL-6 in ileal mucosa of burned mice were much higher than those of control mice, especially at 6 h post-burn (Fig. 4a, b). However, the contents of anti-inflammatory cytokines IL-4 and IL-13 in ileal mucosa of burned mice were dramatically lower than those of control mice (Fig. 4c, d). Importantly, anti-inflammatory cytokine IL-10 showed slight alteration without statistical significance. These results indicate that severe burn could motivate the inflammation in intestinal mucosa, which may be the prominent contributor of intestinal barrier impairment in the early stage of severe burn injury.
Severe burn decreased fecal SCFAs contents
It has been demonstrated that SCFAs act not only as the dominant energy resources of intestinal epithelia but also as the anti-inflammatory factors . Therefore, to more precisely illuminate the underlying mechanisms of intestinal barrier dysfunction induced by severe burn injury, we next investigated whether severe burn injury was accompanied by the alteration of fecal SCFAs contents. Table 1 and Fig. 5 demonstrated the concrete contents and variation tendencies respectively. The contents of all SCFAs, including acetate, propionate, butyrate, isobutyrate, and isovalerate, decreased gradually from 1 h to 7 days post-burn, and dropped to the minimum on 7 days. Thus, severe burn injury could statistically downregulate the contents of intestinal SCFAs, which might contribute to the intestinal inflammation and barrier dysfunction.
Sequencing coverage and measurement of bacterial diversity
It has been illuminated that SCFAs are metabolites of intestinal microbiota . To further identify the mechanisms of severe burn-induced intestinal barrier dysfunction, we next evaluated whether severe burn injury could influence intestinal microbiota composition utilizing an Illumina high-throughput sequencing technique. We created a dataset which is composed of 1,443,620 filtered high-quality and classifiable 16S rDNA gene sequences. The average sequences number of each sample was 36,090.5 (range from 30,093 to 44,839). All sequences were clustered with representative sequences, and a 97% sequence identification cutoff was used. The obtained total number of operational taxonomic units (OTUs) was 11,878. For each sample, bacterial species richness leveled off as sampling depth increased (Additional file 1: Figure S1), indicating that the sequencing effort was sufficiently and that the total diversity within the samples was captured. As shown in Table 2, the microbial richness decreased significantly on 5 days post-burn as compared with the control (p = 0.034). A diversity analysis based on Shannon and Chao  indexes revealed that the diversity of the intestinal microbiota at the OTU level was significantly lower than that of control at 1 h (p = 0.037), 5 days (p = 0.031), and 7 days (p = 0.036) post-burn. These results confirm that severe burn injury remarkably decreases the diversity and richness of intestinal microbiota.
Severe burn disrupted intestinal microbiota
To further understand the alterations of intestinal microbiota after severe burn injury, we next analyzed the intestinal bacterial composition structure in burned mice. As illustrated in Fig. 6, Bacteroidetes, Firmicutes, and Proteobacteria were the three dominant bacteria on phylum level, accounting for 46.39%, 38.88%, and 10.82% of the total sequences, respectively. As showed in Fig. 6 and Additional file 2: Figure S2, the relative abundance of Firmicutes, Bacteroidetes, and Deferribacteres varied a lot among groups. In detail, Bacteroidetes declined in the 3-day and 5-day groups; however, Firmicutes and Deferribacteres elevated in the 3-day and 5-day groups. These results indicate that severe burn injury can obviously change the structure of intestinal microbiota.
Supervised comparison of intestinal microbiota
Based on the community analysis of each sample, we further re-divided these 40 samples into three groups, i.e., control group (N-1 to N-5), burn_early group (1H-1 to 1H-6, 6H-1 to 6H-6, 1D-1 to 1D-6), and burn_late group (3D-1 to 3D-6, 5D-1 to 5D-4, 7D-1 to 7D-6), attempting to highlight the species with different abundance among groups. The results from the principal coordinate analysis (PcoA)  showed the considerable discrepancies in microbial composition at OTU level among the three groups (Additional file 3: Figure S3). Furthermore, we analyzed the compositional differences of intestinal microbiota by utilizing linear discriminant analysis effect size, which is a traditional method for bacterial differential analysis . As indicated in Fig. 7, we discovered that g_Tyzzerella, g_Lachnoclostridium, g_Anaerovorax, g_Ruinococcus_1, g_Lactobacillus, f_Lactobacillaceae, and other 10 species had statistical differences in control group. c_Erysipelotrichia and o_Erysipelotrichales were the discrepant species in the burn_early group. c_Clostridia, g_Bilophila, g_Actinobacillus, g_Pasteurellaceae, and other 11 species were the noticeably varied bacteria in the burn_late group. These results indicate that severe burn is capable of disrupting intestinal microbiota, especially during the late stage of burn injury.
Potential biomarkers analysis
Based on the LefSE analysis, we further utilized the Wilcoxon rank sum test to figure out the potential biomarkers in burned mice. As shown in Fig. 8a, the specific differential bacteria in the burn_early group were norank_Ruminococcaceae (p = 0.02), prevotellaceae_UCG-001 (p = 0.012), Oscillibacter (p = 0.03), and Bacteroides (p = 0.02). However, as illustrated in Fig. 8b, the specific differential bacteria in the burn_late group were norank_Ruminococcaceae (p = 0.004), Alistipes (p = 0.008), and norank_Bacteroidales_S24-7_group (p = 0.01). Thus, these results indicate that these remarkably altered bacteria species may be considered as the potential biomarkers following severe burn injury.
Correlations between intestinal microbial community and environmental factors in severe burn
To address the mutual relationship between specific bacteria species (top 50 species in abundance) and environmental factors, we employed the Spearman correlation analysis in this study. In this part, the SCFAs’ contents and intestinal permeability were regarded as environmental factors. As shown in Fig. 9, the intestinal permeability was positively correlated with Coprococcus_1 (R = 0.459), Anaerotruncus (R = 0.365), Roseburia (R = 0.37), Ruminiclostridium_5 (R = 0.327), and Ruminiclostridium (R = 0.367), but negatively correlated with Desulfovibrio (R = − 0.322) and Prevotellaceae_UCG-001 (R = − 0.331). Among the SCFAs, isobutyric acid was positively correlated with Lachnospiraceae_UCG-005 (R = 0.326), Tyzzerella (R = 0.516), Lactobacillus (R = 0.37), norank_o_Mollicutes_RF9 (R = 0.461), and Akkermansia (R = 0.367). Isovaleric acid was positively correlated with Ruminococcaceae_UCG-014 (R = 0.405), Tyzzerella (R = 0.5), Lactobacillus (R = 0.564), norank_o_Mollicutes_RF9 (R = 0.598), Akkermansia (R = 0.382), and norank_f_Bacteroidales_S24-7_group (R = 0.316), but negatively correlated with Lachnospiraceae_UCG-008 (R = − 0.387). Butyrate was positively correlated with norank_f_Mycoplasmataceae (R = 0.422), but negatively correlated with Escherichia-Shigella (R = − 0.424). Acetate was negatively correlated with unclassified_f_Lchnospiraceae (R = − 0.321) and Bilophila (R = − 0.47), but positively correlated with Ruminocaccaceae_UCG-014 (R = 0.431), norank_o_Mollicutes_RF9 (R = 0.336), and Akkermansia (R = 0.345). Propionate is negatively correlated with Blautia (R = − 0.314), Ruminiclostridium (R = − 0.392) unclassified_f_Lachnospiraceae (R = − 0.34), and norank_f_Ruminococcaceae (R = − 0.396), but positively correlated with Ruminococcaceae_UCG-014 (R = 0.339), Tyzzerella (R = 0.339), norank_f_Mycoplasmataceae (R = 0.327), Lactobacillus (R = 0.435), norank_o_Mollicutes_RF9 (R = 0.399), and unclassified_f_Veillonellaceae (R = 0.347). In brief, norank_o_Mollicutes_RF9, Akkermansia, Lactobacillus, Tyzzerella, and Ruminococcaceae_UCG-014 were the principal species correlated with SCFAs including acetate, propionate, butyrate, isobutyrate, and isovalerate. These results indicate that the variation of intestinal microbiota composition is closely associated with some environmental factors in severe burn injury.
The main original discovery of this study is that severe burn injury disrupts intestinal barrier through affecting the expressions and morphology of tight junction proteins. Meanwhile, the microbial diversity and composition are significantly changed by severe burn injury. Furthermore, severe burn injury also decreases SCFAs’ concentrations and changes inflammatory cytokines’ expressions. These experimental data provides a new insight into the associations among the severe burn-induced intestinal barrier dysfunction, microbiota dysbiosis, inflammatory cytokines, and SCFAs.
It has been well established that severe surgical illness, such as shock, trauma, and burn injury, can destroy intestinal epithelial barrier, resulting in the leakage of bacteria and bacterial metabolites from the intestinal lumen into the mucosa or circulatory system [5, 6, 25]. Based on this study, we identify again that severe burn injury causes intestinal barrier dysfunction, which presents as the increased intestinal permeability, altered tight junction proteins’ expressions, and disrupted ZO-1 morphology. These results are in consistent with the previous studies which show that the burn-induced intestinal barrier disruption is characterized by augmented pare-cellular permeability and altered tight junction proteins’ expressions or morphology [26,27,28]. Thus, there is no doubt that severe burn injury can disrupt the integrity of intestinal epithelial barrier.
Given that severe burn induces intestinal barrier defect, however, the underlying mechanisms are still unclear. Actually, early intestinal disruption caused by burn injury is mainly manifest as a series of pathophysiological events such as inflammation, decreased SCFAs, and intestinal microbiota dysbiosis [29, 30]. It has been reported that the altered intestinal microbiota contributed to augmented intestinal para-cellular permeability . In this study, the intestinal permeability is positively correlated with Coprococcus_1, Anaerotruncus, Roseburia, Ruminiclostridium_5, and Ruminiclostridium, but negatively associated with Desulfovibrio and Prevotellaceae_UCG-001. Thus, the intestinal microbiota dysbiosis may contribute to the occurrence of intestinal barrier disruption induced by severe burn injury. In addition, SCFAs have been reported to be able to enhance intestinal barrier . By the way, SCFAs show protective and stimulative effects on intestinal barrier through inhibiting autophagy and NLRP3 (NLR family, pyrin domain containing protein 3) inflammasome . Therefore, the reduced SCFAs contents observed in present study may also contribute to the severe burn-induced intestinal barrier dysfunction. Furthermore, this study also reveals that the pro-inflammatory cytokines including IL-1β and IL-6 are elevated after severe burn injury, which is consistent with the previous reports [34,35,36]. It is well documented that both IL-1β and IL-6 can disrupt intestinal barrier . Hence, it is rational to speculate that inflammation, intestinal microbiota dysbiosis, and decreased SCFAs contribute to intestinal barrier disruption caused by severe burn injury.
Here, we also show the community-wide changes of intestinal microbiota in severely burned mice. The detailed compositional alterations in the intestinal microbiota following burn injury were investigated at different bacterial taxonomic levels. On phylum level, the predominant phyla were Bacteroidetes, Firmicutes, and Proteobacteria. After severe burn injury, the proportion of Bacteroidetes was decreased, whereas the proportions of Firmicutes, Proteobacteria, and Deferribacteres were increased, resulting in an elevation in Firmicutes/Proteobacteria ratio. On genus level, the genera Mollicutes_RF9_g_norank, Candidatus_Saccharimonas, Butyricimonas, Ruminococcaceae_UCG_010, and Ruminiclostridium_6 were elevated after severe burn. Thus, it is suggested that the decreased microbial diversity estimated by the Shannon Index in present study may be associated with burn-induced inflammatory response, because decreased diversity of intestinal microbial community has been reported in intestinal inflammation .
The composition of individual gut microbiota is believed to be influenced by various factors, such as host genetic elements, immune responses, antimicrobial substances, microbial interactions, and environmental factors . Therefore, based on the observed shifts in bacterial community after burn injury, we further investigated the potential changes of intestinal environmental and fermentative factors. The contents of luminal SCFAs including acetate, propionate, butyrate, isobutyrate, and isovalerate were significantly decreased after severe burn. Similarly, other investigators have also shown that burn injury decreases butyrate contents in the colon of burned mice . Although the mechanism involved in burn decreased SCFAs contents is not clear, it has been documented that decrease in Firmicutes/Proteobacteria ratio leads to increased SCFAs contents . Thus, it is rational to speculate that an elevation in Firmicutes/Proteobacteria ratio observed in this study may be an important cause of the reduced SCFAs contents after severe burn injury.
This study also demonstrates the relationship between specific species of intestinal microbial community and variations of SCFAs contents following severe burn injury. The principal species correlated with SCFAs contents after severe burn injury were Lactobacillus, Akkermansia, Tyzzerella, norank_o_Mollicutes_RF9, and Ruminococcaceae_UCG-014. It has been documented that Ruminococcaceae can produce acetate , and Lactobacillus is able to produce lactate which can be utilized by the bacteria belonging to the Clostridial cluster XIVa to produce butyrate . Besides, the contents of acetate, butyrate, and propionate have been reported to be positively correlated with lactic acid bacteria such as Bacillales, Sporolactobacillus, and Lactobacillus . Thus, our present data, which shows the correlations between bacteria species and SCFAs contents, may provide some implications for understanding the association between intestinal microbiota composition and SCFAs production after severe burn injury.
In conclusion, our present study reveals the variation tendencies of intestinal barrier, microbiota, SCFAs contents, and inflammatory cytokines expressions after severe burn injury. However, the exact relationship between intestinal microbiota dysbiosis and barrier dysfunction following severe burn needs further investigations. A deeper understanding of host-microbial crosstalk might be helpful to the development of novel alternative strategies as well as approaches to restore intestinal barrier after severe burn injury.
Fluorescein isothiocyanate-labeled dextran
Headspace gas chromatography-mass spectrometry
Operational taxonomic unit
Phosphate buffer saline
Principal coordinates analysis
Short-chain fatty acid
Single ion monitoring
Total body surface area
Turner JR. Intestinal mucosal barrier function in health and disease. Nat Rev Immunol. 2009;9(11):799–809.
Shen L, Weber CR, Raleigh DR, Yu D, Turner JR. Tight junction pore and leak pathways: a dynamic duo. Annu Rev Physiol. 2011;73:283–309.
Weber CR. Dynamic properties of the tight junction barrier. Ann N Y Acad Sci. 2012;1257:77–84.
Suzuki T. Regulation of intestinal epithelial permeability by tight junctions. Cell Mol Life Sci. 2013;70(4):631–59.
Deitch EA. Bacterial translocation or lymphatic drainage of toxic products from the gut: what is important in human beings? Surgery. 2002;131(3):241–4.
Magnotti LJ, Deitch EA. Burns, bacterial translocation, gut barrier function, and failure. J Burn Care Rehabil. 2005;26(5):383–91.
Clark A, Imran J, Madni T, Wolf SE. Nutrition and metabolism in burn patients. Burns Trauma. 2017;5:11.
Sekirov I, Russell SL, Antunes LCM, Finlay BB. Gut microbiota in health and disease. Physiol Rev. 2010;90(3):859–904.
Kamada N, Chen GY, Inohara N, Núñez G. Control of pathogens and pathobionts by the gut microbiota. Nat Immunol. 2013;14(7):685–90.
Wang F, Li Q, Wang C, Tang C, Li J. Dynamic alteration of the colonic microbiota in intestinal ischemia-reperfusion injury. PLoS One. 2012;7(7):e42027.
Cushing K, Alvarado DM, Ciorba MA. Butyrate and mucosal inflammation: new scientific evidence supports clinical observation. Clin Transl Gastroenterol. 2015;6:e108.
Arpaia N, Campbell C, Fan X, Dikiy S, van der Veeken J, deRoos P, et al. Metabolites produced by commensal bacteria promote peripheral regulatory T-cell generation. Nature. 2013;504(7480):451–5.
Furusawa Y, Obata Y, Fukuda S, Endo TA, Nakato G, Takahashi D, et al. Commensal microbe-derived butyrate induces the differentiation of colonic regulatory T cells. Nature. 2013;504(7480):446–50.
Chang PV, Hao L, Offermanns S, Medzhitov R. The microbial metabolite butyrate regulates intestinal macrophage function via histone deacetylase inhibition. Proc Natl Acad Sci. 2014;111(6):2247–52.
Singh N, Gurav A, Sivaprakasam S, Brady E, Padia R, Shi H, et al. Activation of Gpr109a, receptor for niacin and the commensal metabolite butyrate, suppresses colonic inflammation and carcinogenesis. Immunity. 2014;40(1):128–39.
Kelly CJ, Zheng L, Campbell EL, Saeedi B, Scholz CC, Bayless AJ, et al. Crosstalk between microbiota-derived short-chain fatty acids and intestinal epithelial HIF augments tissue barrier function. Cell Host Microbe. 2015;17(5):662–71.
Koh A, De Vadder F, Kovatcheva-Datchary P, Bäckhed F. From dietary fiber to host physiology: short-chain fatty acids as key bacterial metabolites. Cell. 2016;165(6):1332–45.
Braniste V, Al-Asmakh M, Kowal C, Anuar F, Abbaspour A, Tóth M, et al. The gut microbiota influences blood-brain barrier permeability in mice. Sci Transl Med. 2014;6(263):263ra158.
Huang YL, Feng YH, Wang Y, Wang P, Wang FJ, Ren H. Severe burn-induced intestinal epithelial barrier dysfunction is associated with endoplasmic reticulum stress and autophagy in mice. Front Physiol. 2018;9:441.
Amato KR, Yeoman CJ, Kent A, Righini N, Carbonero F, Estrada A, et al. Habitat degradation impacts black howler monkey (Alouatta pigra) gastrointestinal microbiomes. ISME J. 2013;7(7):1344–53.
Krause G, Winkler L, Mueller SL, Haseloff RF, Piontek J, Blasig IE. Structure and function of claudins. Biochim Biophys Acta (BBA). 2008;1778(3):631–45.
Schloss PD, Gevers D, Westcott SL. Reducing the effects of PCR amplification and sequencing artifacts on 16S rRNA-based studies. PLoS One. 2011;6(12):e27310.
Jiang XT, Peng X, Deng GH, Sheng HF, Wang Y, Zhou HW, et al. Illumina sequencing of 16S rRNA tag revealed spatial variations of bacterial communities in a mangrove wetland. Microb Ecol. 2013;66:96–104.
Zhang C, Li S, Liu Yang LW, Wang S, Zhao G, et al. Structural modulation of gut microbiota in life-long calorie-restricted mice. Nat Commun. 2013;4:2163.
Leaphart CL, Tepas JJ. The gut is a motor of organ system dysfunction. Surgery. 2007;141(5):563–9.
Costantini TW, Loomis WH, Putnam JG, Drusinsky D, Deree J, Choi S, et al. Burn-induced gut barrier injury is attenuated by phosphodiesterase inhibition. Shock. 2009;31(4):416–22.
Chen C, Wang P, Su Q, Wang S, Wang F. Myosin light chain kinase mediates intestinal barrier disruption following burn injury. PLoS One. 2012;7(4):e34946.
Hammer AM, Khan OM, Morris NL, Li X, Movtchan NV, Cannon AR, et al. The effects of alcohol intoxication and burn injury on the expression of claudins and mucins in the small and large intestines. Shock. 2016;45(1):73–81.
Shimizu K, Oqura H, Asahara T, Nomoko K, Matsushima A, Hayakawa K, et al. Gut microbiota and environment in patients with major burns-a preliminary report. Burns. 2015;41(3):e28–33.
Earley ZM, Akhtar S, Green SJ, Naqib A, Khan O, Cannon AR, et al. Burn injury alters the intestinal microbiome and increases gut permeability and bacterial translocation. PLoS One. 2015;10(7):e0129996.
Xavier RJ, Podolsky DK. Unravelling the pathogenesis of inflammatory bowel disease. Nature. 2007;448(7152):427–34.
Elamin EE, Masclee AA, Dekker J, Pieters HJ, Jonkers DM. Short-chain fatty acids activate AMP-activated protein kinase and ameliorate ethanol-induced intestinal barrier dysfunction in Caco-2 cell monolayers. J Nutr. 2013;143(12):1872–81.
Feng Y, Wang Y, Wang P, Huang Y, Wang F. Short-chain fatty acids manifest stimulative and protective effects on intestinal barrier function through the inhibition of NLRP3 inflammasome and autophagy. Cell Physiol Biochem. 2018;49(1):190–205.
Zhu L, Liu X, Du L, Jin Y. Preparation of asiaticoside-loaded coaxially electrospinning nanofibers and their effect on deep partial-thickness burn injury. Biomed Pharmacother. 2016;83:33–40.
Yun J, Cho K. Effects of organic loading rate on hydrogen and volatile fatty acid production and microbial community during acidogenic hydrogenesis in a continuous stirred tank reactor using molasses wastewater. J Appl Microbiol. 2016;121:1627–36.
Gan HT, Pasricha PJ, Chen JD. Blockade of p38 mitogen-activated protein kinase pathway ameliorates delayed intestinal transit in burned rats. Am J Surg. 2007;193(4):530–7.
Suzuki T, Yoshinaga N, Tanabe S. Interleukin-6 (IL-6) regulates claudin-2 expression and tight junction permeability in intestinal epithelium. J Biol Chem. 2011;286(36):31263–71.
Nagao-Kitamoto H, Shreiner AB, Gillilland MG, Kitamoto S, Ishii C, Hirayama A, et al. Functional characterization of inflammatory bowel disease–associated gut dysbiosis in gnotobiotic mice. Cell Mol Gastroenterol Hepatol. 2016;2(4):468–81.
Gentschew L, Ferguson LR. Role of nutrition and microbiota in susceptibility to inflammatory bowel diseases. Mol Nutr Food Res. 2012;56(4):524–35.
Kuethe JW, Armocida SM, Midura EF, Rice TC, Hildeman DA, Healy DP, et al. Fecal microbiota transplant restores mucosal integrity in a murine model of burn injury. Shock. 2016;45:647–52.
Sheflin AM, Borresen EC, Kirkwood JS, Boot CM, Whitney AK, Lu S, et al. Dietary supplementation with rice bran or navy bean alters gut bacterial metabolism in colorectal cancer survivors. Mol Nutr Food Res. 2017;61(1):1.
Chassard C, Bernalier-Donadille A. H2 and acetate transfers during xylan fermentation betweena butyrate-producingxylanolytic species and hydrogenotrophic microorganisms from the human gut. FEMS Microbiol Lett. 2005;254:116–22.
Muñoz-Tamayo R, Laroche B, Walter E, Doré J, Duncan SH, Flint HJ. Kinetic modelling of lactate utilization and butyrate production by key human colonic bacterial species. FEMS Microbiol Ecol. 2011;76(3):615–24.
We appreciate the central laboratory of the third military medical university (Army medical university) and Majorbio company (China) for technological support.
This work was supported by the National Natural Science Foundation of China (81772081).
Availability of data and materials
All data generated or analyzed during this study are included in this published article.
Ethics approval and consent to participate
The animal studies were approved by the Animal Care and Use Committee of Third Military Medical University (Army Medical University), and all the protocols were approved by the Medical and Ethics Committee of Southwest Hospital, Third Military Medical University (Army Medical University), Chongqing, China.
Consent for publication
The authors declare that they have no competing interests.
Figure S1. Rarefaction curve of the fecal samples (97% similarity). Repeated samples of operational taxonomic unit (OTU) subsets were used to evaluate whether further sampling would likely yield additional taxa, as indicated by whether the curve has reached a plateau value. N stands for control group, 1H, 6H stands for 1-h, 6-h post-burn group, 1D, 3D, 5D, 7D stands for 1-day, 3-day, 5-day, 7-day post-burn group. (TIF 1401 kb)
Figure S2. Abundance alteration of specific bacteria on Phylum level. Abundance of each bacteria on Phylum level was assessed in this experiment. The X-axis is grouping information, and the Y-axis represents the abundance of species on Phylum level. After burn injury, the abundance of Bacteroidetes decreased significantly at 3 days and 5 days; however, abundance of Firmicutes and Deferribacteres increased at 3 days and 5 days. Data represent the mean ± standard error of the mean (SEM) (n = 4–6). *p < 0.05 compared with control, Dunnett's t test was used for analysis. Ctrl stands for control group, 1H, 6H stands for 1-h, 6-h post-burn group, 1D, 3D, 5D, 7D stands for 1-day, 3-day, 5-day, 7-day post-burn group. (TIF 254 kb)
Figure S3. Principal coordinates analysis (PCoA) using weighted unifrac. The green dots indicate the distributions of samples in the control group. The red triangles stand for samples in burn_early group. The blue quadrangles represent the specimens in the burn_late group. OTU operational taxonomic unit. (TIF 244 kb)
About this article
Cite this article
Feng, Y., Huang, Y., Wang, Y. et al. Severe burn injury alters intestinal microbiota composition and impairs intestinal barrier in mice. Burn Trauma 7, 20 (2019). https://doi.org/10.1186/s41038-019-0156-1
- Intestinal barrier
- Tight junction protein
- Intestinal microbiota
- Short-chain fatty acids
- Inflammatory cytokines