Objective Antimicrobial C-type lectin regenerating islet-derived 3 gamma (REG3G) is suppressed in the small intestine during chronic ethanol feeding. Our aim was to determine the mechanism that underlies REG3G suppression during experimental alcoholic liver disease.
Design Interleukin 22 (IL-22) regulates expression of REG3G. Therefore, we investigated the role of IL-22 in mice subjected to chronic-binge ethanol feeding (NIAAA model).
Results In a mouse model of alcoholic liver disease, we found that type 3 innate lymphoid cells produce lower levels of IL-22. Reduced IL-22 production was the result of ethanol-induced dysbiosis and lower intestinal levels of indole-3-acetic acid (IAA), a microbiota-derived ligand of the aryl hydrocarbon receptor (AHR), which regulates expression of IL-22. Importantly, faecal levels of IAA were also found to be lower in patients with alcoholic hepatitis compared with healthy controls. Supplementation to restore intestinal levels of IAA protected mice from ethanol-induced steatohepatitis by inducing intestinal expression of IL-22 and REG3G, which prevented translocation of bacteria to liver. We engineered Lactobacillus reuteri to produce IL-22 (L. reuteri/IL-22) and fed them to mice along with the ethanol diet; these mice had reduced liver damage, inflammation and bacterial translocation to the liver compared with mice fed an isogenic control strain and upregulated expression of REG3G in intestine. However, L. reuteri/IL-22 did not reduce ethanol-induced liver disease in Reg3g–/– mice.
Conclusion Ethanol-associated dysbiosis reduces levels of IAA and activation of the AHR to decrease expression of IL-22 in the intestine, leading to reduced expression of REG3G; this results in bacterial translocation to the liver and steatohepatitis. Bacteria engineered to produce IL-22 induce expression of REG3G to reduce ethanol-induced steatohepatitis.
- immune response
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Significance of this study
What is already known on this subject?
Alcoholic liver disease (ALD) is characterised by intestinal dysbiosis.
Chronic ethanol feeding reduces intestinal expression of regenerating islet-derived 3 gamma (REG3G) in mice and humans.
REG3G is protective against ethanol-induced liver injury.
Intestinal Reg3g expression is mediated by interleukin 22 (IL-22).
What are the new findings?
Ethanol feeding causes impaired IL-22 production by ILC3s in the gut, which is the result of ethanol-induced dysbiosis and lower intestinal levels of indole-3-acetic acid (IAA), a microbiota-dependent aryl hydrocarbon receptor ligand.
Patients with alcoholic hepatitis have lower faecal IAA levels compared with healthy controls.
IAA supplementation restores Il22 and Reg3g expression and protects from ethanol-induced steatohepatitis.
IL-22 producing engineered bacteria ameliorate experimental ALD via Reg3g induction.
How might it impact on clinical practice in the foreseeable future?
Engineered IL-22-producing bacteria can be used as therapeutics for alcohol-induced liver disease.
Alcoholic liver disease affects several million people worldwide and can progress from hepatic steatosis and alcoholic steatohepatitis to cirrhosis and hepatocellular carcinoma.1 In 2010, alcohol-attributable chronic liver disease was responsible for almost 500 000 deaths globally. Chronic alcohol intake contributes to gut barrier dysfunction, increased intestinal permeability and changes in gut microbiota composition (dysbiosis).2 Moreover, transplantation of gut microbiota from patients with alcoholic hepatitis to mice demonstrated that alcohol-associated dysbiosis contributes to the development of severe liver disease and is transmissible, through faecal microbiota transfer.3
C-type lectins mediate the intestinal immune response against pathogens and maintain homeostasis of commensal microbes.4 One C-type lectin, regenerating islet-derived 3 gamma (REG3G), is primarily expressed in the small intestine. Levels of REG3G are reduced in small intestines of mice after chronic ethanol feeding and in the duodenum of patients with alcohol use disorder.5 6 Reg3g –/– mice have increased susceptibility to ethanol-induced liver disease, in association with increased translocation of bacteria to the liver.7 However, intestine-specific overexpression of REG3G protects mice against ethanol-induced liver disease by reducing bacterial translocation. However, the mechanism by which chronic ethanol feeding reduces intestinal expression of REG3G and increases bacterial translocation is unknown.
The production of REG3G lectins is regulated by interleukin 22 (IL-22), a cytokine mainly expressed by RORγt+ type 3 innate lymphoid cells (ILC3) in the gut during homeostasis.8 Here, we investigated whether ethanol-induced dysbiosis impairs IL-22 production in the gut and expression of REG3G to promote bacterial translocation and liver disease. We also tested the effects of IL-22-producing bioengineered bacteria on ethanol-induced liver disease in mice.
Chronic–binge ethanol feeding reduces intestinal production of IL-22 by ILC3 in mice
Chronic alcohol feeding reduces intestinal levels of Reg3g mRNA and protein in mice and humans.5 6 We performed studies with chronic–binge ethanol-fed mice as a model of alcoholic steatohepatitis.9 These mice had significant increases in mean plasma level of alanine aminotransferase (ALT) and hepatic level of triglycerides (figure 1A–C) and a reduced level of Reg3g and Reg3b mRNA in the small intestinal epithelium compared with pair-fed mice on an isocaloric diet (controls) (figure 1D,E). The expression of other antimicrobial proteins defensin alpha 3 (Defcr3), defensin alpha 5 (Defcr5), S100a8 and lipocalin 2 (Lcn2) in the small intestine was not changed (see online supplementary figure S1a). As the expression of Reg3g can be modulated via recognition of bacterial ligands by Toll-like receptor 4 (TLR4)10 and subsequent MyD88 activation,11 Tlr4 and Myd88 mRNA levels were assessed in small intestinal epithelial cells. No difference was observed in the expression levels of Tlr4 and MyD88 between ethanol-fed and isocaloric-fed mice (see online supplementary figure S1a). Yet, the ethanol-fed mice had a significant decrease in level of Il22 mRNA in total lamina propria cells of the small intestine compared with controls (figure 1F). In addition, the frequency of IL-22-expressing ILC3 (gated on CD3−RORγt+) was significantly reduced in ethanol-fed mice compared with controls (figure 1G), while expression of the IL-22 receptor subunit alpha 1 (Il22Ra1) in small intestinal epithelium did not differ (see online supplementary figure S1a). Furthermore, increased expression of interleukin 1 beta (Il1b) and interleukin 18 (Il18) were found in small intestine of chronic-binge ethanol-fed mice compared with controls, while interleukin 10 (Il10), another IL-10 family member, and interleukin 25 (Il25), which is able to repress IL-22 production by RORγt+ ILC3s,12 13 did not change (see online supplementary figure S1b).
To determine whether the reduction in IL-22 expression is a direct effect of ethanol, we measured IL-22 expression in lamina propria cells that were either preincubated for 1 hour or coincubated for 4 hours with ethanol (50 mM or 100 mM) during IL-23 stimulation. Levels of Il22 mRNA and the frequency of IL-22+ ILC3 did not differ between cells incubated with ethanol or under control conditions (see online supplementary figure S2a–d). These findings provide evidence that ethanol indirectly reduces IL-22 expression by ILC3 in the gut, thereby reducing expression of REG3G and REG3B.
Intestinal levels of indole-3-acetic acid (IAA) are reduced during ethanol feeding in mice and in patients with alcoholic hepatitis
Alterations in the gut microbiota composition and bacterial overgrowth (dysbiosis), intestinal barrier dysfunction and bacterial translocation have been implicated in development of alcoholic liver disease.9 Microbiota can modulate IL-22 production via production of metabolites from tryptophan catabolism, called indoles, which are ligands for the aryl-hydrocarbon receptor (AHR).14 In line with results from AHR-deficient mice,15 we observed reduced Il22 expression in ILC3 on incubation with an AHR inhibitor (CH223191), indicating that IL-22 production by lamina propria cells in the small intestine requires AHR (figure 2A).
We therefore measured intestinal levels of metabolites described as potent activators of AHR in mice after chronic–binge ethanol feeding or the control diet using targeted metabolomics. Mice on the chronic–binge ethanol diet had lower mean amounts of IAA (figure 2B), a microbiota-dependent AHR ligand16 and indole-3-sulfate (figure 2C) in the small intestine. Levels of other potential AHR ligands such as tryptamine (figure 2D), indole-3-aldehyde (figure 2E), indole-3-acetamide (figure 2F), a precursor of IAA and indole-3-lactic acid17 (figure 2G) did not differ significantly between mice fed the ethanol versus the control diet. These data indicate that ethanol feeding reduces microbiota-dependent production of AHR ligands from tryptophan, which could be responsible for the reduced IL-22 production.
To validate our findings in a clinical setting, levels of microbiota-dependent AHR ligands were determined in stool samples from patients with alcoholic hepatitis (n=13) and healthy controls (n=17). Similar to our findings in mice, faecal levels of IAA were significantly reduced in patients with alcoholic hepatitis compared with controls (figure 2H). In addition, indole-3-lactic acid was lower in faeces from patients with alcoholic hepatitis (figure 2I). These data supports that ethanol consumption alters tryptophan catabolism, thereby potentially affecting antimicrobial defense mechanisms by Reg3 lectins.
Supplementation with IAA reduces ethanol-induced steatohepatitis
Since intestinal IAA levels were reduced in both, patients with alcoholic hepatitis and mice fed a chronic-binge ethanol diet, we aimed to restore intestinal levels of IAA by oral supplementation to mice. Daily oral administration of IAA (20 mM) during chronic–binge ethanol feeding decreased liver damage and steatosis, indicated by the significant reductions in plasma levels of ALT and hepatic levels of triglyceride (figure 3A–C), whereas liver-to-body weight ratio was unchanged (see online supplementary figure S3a). IAA administration did not affect plasma levels of ethanol or hepatic expression of Cyp2e1 and Adh1 mRNAs, which regulate hepatic metabolism of ethanol (see online supplementary figure S3b–d). Supplementation with IAA restored expression of Il22 and Reg3g mRNAs in small intestine compared with control mice (figure 3D,E).
IAA supplementation prevented ethanol-induced translocation of bacteria to liver (figure 3F). Moreover, hepatic expression of genes regulated by AHR, Cyp1a1 and Cyp1b1 did not change significantly during IAA supplementation, indicating no significant systemic effects of IAA on AHR signalling in liver (see online supplementary figure S3e,f). So, defects in AHR-mediated expression of IL-22, resulting from reduced production of IAA, contribute to ethanol-induced steatohepatitis.
Alcohol-associated dysbiosis decreases intestinal IL-22 production
To test whether the microbiome is involved in reducing the expression of IL-22, we analysed production of IL-22 by ILC3 in small intestinal lamina propria cells of mice given non-absorbable antibiotics, which prevent alcohol-associated intestinal bacterial overgrowth and dysbiosis.18 19 Importantly, the antibiotics used in our approach (Polymyxin B and Neomycin) predominantly target aerobic Gram-negative bacteria (so mostly Enterobacteriaceae), thereby not removing all bacterial strains.20
In line with our previous findings,18 19 administration of non-absorbable antibiotics prevented development of ethanol-induced steatohepatitis in mice, indicated by reduced mean plasma levels of ALT and hepatic levels of triglycerides (figure 4A–C) and restored liver-to-body weight ratio (see online supplementary figure S4a). We found no changes in plasma levels of ethanol (see online supplementary figure S4b) or hepatic expression of Cyp2e1 or Adh1 genes (see online supplementary figure S4c,d). The prevention of liver damage by non-absorbable antibiotics was associated with restored expression of Il22 mRNA in lamina propria cells and IL-22 production by ILC3 on IL-23 stimulation (figure 4D,E). Mechanistically, we observed that antibiotics treatment was associated with increased intestinal levels of the AHR ligand indole-3-lactic acid,17 while IAA and indole-3-aldehyde levels did not significantly change (see online supplementary figure S4e–g). These data support that impaired intestinal IL-22 production results from ethanol-associated dysbiosis causing altered tryptophan catabolism and AHR ligand production.
Bacteria engineered to produce IL-22 reduce ethanol-induced steatohepatitis and bacterial translocation
With an aim to restore intestinal expression of IL-22 in our mouse model of alcoholic liver disease, we developed a strain of Lactobacillus reuteri that produces mouse IL-22 (L. reuteri/IL-22). IL-22 was only present in supernatants of overnight cultures of the engineered L. reuteri/IL-22 strain (see online supplementary figure S5a). Mice were given daily phosphate-buffered saline (PBS; control), isogenic L. reuteri (bacteria control) or L. reuteri/IL-22 (107 CFU/day) by oral gavage during 10 days of chronic–binge ethanol feeding. Daily administration was necessary, given that L. reuteri does not colonise mice (see online supplementary figure S5b). Systemic IL-22 administration to mice reduces ethanol-induced liver disease and acute ethanol-induced hepatotoxicity.21 22 We therefore titrated bacteria so that we would not observe increased systemic levels of IL-22. Administration of L. reuteri or L. reuteri/IL-22 to mice did not affect their levels of IL-22 in the circulation, suggesting an intestine-restricted effect (figure 5A). However, administration of L. reuteri/IL-22 significantly reduced steatohepatitis (figure 5B–D) and decreased levels of Cxcl1 and Cxcl2 mRNAs, compared with controls (figure 5E,F). Liver-to-body weight ratio was unaffected by bacteria (see online supplementary figure S5c).
To evaluate effects on ethanol metabolism, we measured plasma levels of ethanol and hepatic expression of Cyp2e1 and Adh1. We found no differences among groups of mice, indicating that the protective effect of L. reuteri/IL-22 is independent of changes in ethanol metabolism (see online supplementary figure S5d–f). Compared with controls, we found L. reuteri/IL-22 administration increased expression of Reg3g mRNA in the small intestine of ethanol-fed mice (figure 5G). Although a trend towards an increase in Reg3b mRNA was observed in the small intestine of L. reuteri/IL-22-treated mice, no significant difference was seen in the expression levels compared with controls (see online supplementary figure S5g). Similarly, expression of Defcr3 and Defcr5 was unchanged (see online supplementary figure S5g). L. reuteri/IL-22 also significantly reduced bacterial translocation to the liver during chronic–binge ethanol feeding, compared with the bacteria control (figure 5H). Unaltered Occludin mRNA levels indicate no effect on tight junctions in the small intestine of our bacteria-based IL-22 treatment (see online supplementary figure S5g). Moreover, no differences were found in IL-22 production by ILC3 and Il22 mRNA in lamina propria cells between mice treated with PBS, L. reuteri and L. reuteri/IL-22 (see online supplementary figure S6a,b). L. reuteri/IL-22 treatment did not affect intestinal IAA, indole-3-lactic acid and indole-3-aldehyde levels (see online supplementary figure S6c–e). Our engineered L. reuteri was therefore able to restore intestinal levels of IL-22 in mice during chronic–binge ethanol feeding—the bacterially expressed IL-22 led to re-expression of REG3G, reduced bacterial translocation and ethanol-induced steatohepatitis.
No effects of L. reuteri/IL-22 on liver disease in REG3G-deficient mice
We studied development of liver disease in chronic–binge ethanol-fed Reg3g –/– mice gavaged with L. reuteri/IL-22 or controls and their wild type littermates. Consistent with our previously published data using a chronic Lieber DeCarli ethanol feeding model for 8 weeks,7 mice deficient for REG3G developed more ethanol-induced liver disease as indicated by increased plasma ALT levels, hepatic triglycerides and inflammation and bacterial translocation to the liver (figure 6A–F). Wild-type mice gavaged with L. reuteri/IL-22 showed ameliorated ethanol-induced liver disease, increased Reg3g expression in the small intestine and reduced bacterial translocation to the liver (figure 6A– F). We did not observe a reduction in ethanol-induced steatohepatitis in Reg3g –/– mice given L. reuteri/IL-22 (figure 6A–C), and hepatic levels of Cxcl1 mRNAs did not differ significantly in mice fed L. reuteri/IL-22 vs controls (figure 6D). Moreover, equal amounts of bacteria were translocated to the livers of mice fed L. reuteri/IL-22 versus controls (figure 6F). There were no significant differences between groups of mice in liver-to-body weight ratio, plasma levels of ethanol or hepatic expression of Cyp2e1 and Adh1 mRNAs (see online supplementary figure S7a–d). These findings indicate that the protective effect of intestinal IL-22 supplementation depends on intestinal REG3G.
Changes in genetic, environmental, and dietary factors, as well as alcohol abuse, contribute to intestinal dysbiosis.23 24 Nevertheless, the precise mechanism by which alcohol-induced gut dysbiosis causes liver disease are poorly understood. Chronic ethanol feeding reduces expression of REG3G in the small intestine, increasing translocation of bacteria to liver and progression of liver disease.5 6 It has not been clear how REG3G expression is downregulated in mice with ethanol-induced liver disease.
We found that ethanol reduces intestinal production of IL-22 by altering microbial catabolism of tryptophan into AHR ligands. Restoration of intestinal IL-22, by administration of the AHR ligand IAA or via engineered bacteria, reduces ethanol-induced steatohepatitis by inducing expression of intestinal REG3G, which reduces bacterial translocation to the liver (figure 7). Moreover, the reduction in intestinal IAA levels was consistent in patients diagnosed with alcoholic hepatitis compared with healthy controls. These findings indicate the importance of AHR signalling to IL-22 to sustain expression of REG3G in the gut during alcoholic liver disease.
Various immune cells produce IL-22. Non-lymphoid sources, such as macrophages, neutrophils, and dendritic cells, produce less IL-22 compared with lymphoid sources, such as αβ and γδT cells, natural killer T cells and innate lymphoid cells (ILC).12 In the intestine, type 3 ILC are a major source of IL-22; production depends on cytokines secreted from myeloid cells, mainly IL-23 and IL-1B.25
Production of IL-22 by ILC is influenced by microbiota.26 For example, commensal bacteria can suppress intestinal RORγt+ILC production of IL-22 in healthy mice.27 In addition, germ-free mice lack expression of Rorc and Il22 mRNAs in the small intestine lamina propria.28 29 Commensal bacteria affect ILC populations either indirectly, via recognition by resident myeloid or epithelial cells and subsequent cytokine production or by direct recognition of commensal bacteria or commensal bacteria-derived products by toll-like receptors, natural cytotoxicity receptors or the AHR (reviewed in ref 26). Indole derivatives from tryptophan catabolism activate the AHR to modulate local IL-22 production and regulate intestinal barrier function.14 16 Increased AHR signalling inhibits inflammation and colitis in the gastrointestinal tract of mice via production of IL-22.30 Importantly, the availability and production of AHR ligands from tryptophan is controlled by the microbiota.31 Metabolomic analyses indicated that germ-free mice have increased levels of tryptophan in plasma and colon, whereas IAA production was impaired in the lumen of the colons.16 32
Which microbes produce AHR ligands? Indole derivatives are mostly produced by intestinal bacteria with tryptophanase activity.32 For instance, lactobacilli activate ILC3 and production of IL-22 via their production of AHR ligands, thereby providing epithelial protection while inducing resistance against Candida albicans.14 Interestingly, alcohol-dependent patients have overgrowth of Candida, independent of the stage of liver disease.33 Moreover, dysbiosis in ethanol-fed mice is characterised by reduced Lactobacillus,6 whereas several studies demonstrated a beneficial effect of probiotic Lactobacillus strains in rodent models of alcoholic liver disease.34 35 We found that stimulating lactobacilli using prebiotic fructo-oligosaccharides partially restored expression of REG3G, thereby reducing ethanol-induced steatohepatitis in mice.6 In the process of tryptophan catabolism, different bacterial enzymes are responsible for the production of indole derivatives. Our current data suggest that certain bacterial strains responsible for specific AHR ligands (ie, indole-3-lactic acid) were resistant to our antibiotics treatment, thereby potentially restoring intestinal eubiosis and IL-22 function. Further studies are needed to identify which bacterial species specifically produce certain AHR ligands, thereby providing more molecular insights and identify new potential targets for therapy.
The ability of systemic IL-22 to protect against ethanol-induced liver disease has been described before.21 Administration of recombinant IL-22 or an IL-22-expressing adenovirus during chronic–binge ethanol feeding reduced fatty liver, liver injury and hepatic oxidative stress, via activation of STAT3 in the liver.21 We demonstrate that intestine-restricted delivery of IL-22 reduces ethanol-induced steatohepatitis by increasing expression of Reg3g and preventing bacterial translocation to the liver. These data are in line with our previous findings, in which we show that overexpression of REG3G in intestinal epithelial cells reduces bacterial translocation and protects mice from ethanol-induced steatohepatitis.7 In addition to a direct hepato-protective effect of IL-22 during ethanol-induced liver disease, IL-22 has the beneficial effect of reducing bacterial translocation in intestine.
We have shown that bacteria can be engineered to express specific proteins in the intestine, providing evidence that microbes can be manipulated to act as therapeutic agents. Bacteria that are genetically manipulated to produce specific factors might be more effective than systemic administration of agents and produce fewer side effects. For example, systemic administration of IL-22 increases the risk of liver tumours in patients with chronic liver disease.36–38 Studies are needed to determine whether we can increase intestinal AHR signalling with specific AHR ligands, probiotic Lactobacilli strains or bacteria engineered in other ways to reduce progression of alcoholic liver disease. We have identified tryptophan catabolism, an important therapeutic target, and offer a strategy to reverse deficiencies in AHR ligands. Increasing the protective functions of the immune responses by these means could lead to new therapeutic strategies.
C57BL/6 mice were purchased from Charles River and used in all described experiments. Reg3g –/– mice on a C57BL/6 background have been described.39 Heterozygous mice were used for breeding, and wild type and knockout littermate mice were used in all experiments.
Female and male mice (8–12 weeks) were subjected to chronic–binge alcohol feeding (NIAAA) as described previously.9 Mice were fed with Lieber-DeCarli diet for 15 days, starting at day 6 with ethanol feeding. The caloric intake from ethanol was 0% on days 1–5 and 36% from day 6 until the end. At day 16, mice were gavaged with one dose of ethanol (5 g/kg bodyweight) in the morning and sacrificed 9 hours later. Pair-fed control mice received a diet with an isocaloric substitution of dextrose. Antibiotics treatment was started at day 1 of ethanol feeding, and mice were gavaged daily until harvesting. The composition of antibiotics mixture has been described (Polymyxin B (150 mg/kg BW) and Neomycin (200 mg/kg BW)).18 Control mice were gavaged with an equal volume of vehicle (water). Supplementation of IAA was done by daily gavage of 100 µL of 20 mM IAA (initially dissolved in a small volume of NaOH before adjusting with water to prepare the final concentration) or vehicle water, starting at day 1 of ethanol feeding. To study the effect of the engineered bacteria, a volume of 100 µL PBS, L. reuteri (107 CFU/day) or L. reuteri/IL-22 (107 CFU/day) was gavaged daily, starting at day 1 of ethanol feeding. L. reuteri and L. reuteri/IL-22 strains were daily freshly grown in MRS Lactobacilli broth (Sigma), overnight at 37°C.
Non-alcoholic control subjects (n=17; 14 male/3 female; mean age=42) and patients with alcoholic hepatitis (n=13; nine male, four female; mean age=58; average model for end stage liver disease (MELD) score=22) were enrolled. Inclusion and exclusion criteria have been described.40 For metabolomics, faecal samples (10 mg each) were homogenised using Genogrinder at 1500 rpm for 30 s and extracted with 225 µL of −20°C cold, degassed methanol and 750 µL of methyl tertiary butyl ether (Sigma Aldrich, St. Louis, Missouri, USA). One hundred and eighty-eight microlitre of liquid chromatography - mass spectrometry (LC-MS) grade water was then added to the samples to induce phase separation, followed by centrifugation at 14 000 × g for 2 min. The bottom layer (125 µL) was collected, evaporated to dryness and then resuspended in 60 µL 4:1 acetonitrile and water (v/v) with internal standards. Samples were then vortexed, sonicated for 5 min, centrifuged for 2 min at 14 000 × g and prepared for injection. Hydrophilic interaction liquid chromatography with quadrupole time-of-flight mass spectrometry was used for the untargeted metabolomics profiling as described previously.41 Briefly, 2 µL of resuspended sample was injected onto an Acquity UPLC BEH Amide column (150 mm×2.1 mm; 1.7 µm) coupled to an Acquity VanGuard BEH Amide precolumn (5 mm×2.1 mm; 1.7 µm, Waters, Milford, Massachusetts, USA). The column was maintained at 45°C. Agilent 1290 Infinity UHPLC system (Agilent Technologies, Santa Clara, California, USA) coupled to a Sciex TripleTOF 5600+ (SCIEX, Framingham, Massachusetts, USA) was used. Mobile phase A was 100% LC-MS grade water with 10 mM ammonium formate and 0.125% formic acid (Sigma-Aldrich). Mobile phase B was 95:5 v/v acetonitrile:water (v/v) with 10 mM ammonium formate and 0.125% formic acid (Sigma–Aldrich). Gradient was performed as follows: 0–2 min 100% B, 7.7 min 70% B, 9.5 min 40% B, 10.25 min 30% B, 12.75 min 100% B, isocratic until 16.75 min with a flow rate of 0.4 mL/min. Mass spectra were collected in ESI positive mode with data-dependent MS/MS spectra acquisition method. Method blank and human plasma (BioIVT, Westbury, New York, USA) samples were used as quality control samples and injected at the beginning of the run and every 10 samples throughout the run. LC-MS raw data files were converted to ABF format and then processed using MS-DIAL version 2.9442 for deconvolution, peak detection and alignment. Ion adducts, duplicate peaks and isotopic features were identified using MS-FLO.43 In house retention time-m/z library and MS/MS spectra databases were used for compound identification. Features present in at least 50% of samples in each group were reported.
Plasma levels of ethanol were measured using the Ethanol Assay Kit (BioVision). Levels of ALT were determined using Infinity ALT kit (Thermo Scientific). Hepatic triglyceride levels were measured using the Triglyceride Liquid Reagents Kit (Pointe Scientific). Levels of IL-22 in plasma and culture supernatants were determined using the Mouse IL-22 DuoSet ELISA kit according to manufacturer’s protocol (DY582, R&D Systems).
Real-time quantitative PCR
RNA was extracted from mouse tissues, and cDNAs were generated.44 Reverse-transcribed cDNA from tissue or cell culture was amplified on a CFX96 system (Bio-Rad Laboratories) using KAPA SYBR FAST qPCR Kit Master Mix (2X) (KK4606, Kapa Biosystems) and primers for indicated genes. Primer sequences for mouse genes were obtained from the NIH qPrimerDepot. The qPCR value was normalised to 18S.
Bacterial DNA isolation and qPCR for 16S
Histological analysis of liver tissues
For determination of lipid content, livers were embedded in OCT compound, sectioned at 7 µm thickness, and frozen sections were stained with Oil Red O (Sigma-Aldrich). Samples were analysed by densitometry, using NIH Image J software. For quantification, the average percentage area positively stained for each mouse was calculated from at least five random pictures of stained liver sections. The results are presented as percentage area positively stained.
Isolation of lamina propria cells
Small intestines were harvested and placed in ice-cold Hank’s balanced salt solution (HBSS). After removal of residual mesenteric fat tissue, Peyer’s patches were excised, and small intestines were opened longitudinally. Tissues were washed in ice-cold HBSS and cut into 1 cm pieces. Then, tissues were incubated in 20 mL of HBSS with 5 mM EDTA, 1 mM sodium pyruvate, 25 mM HEPES and 1 mM dithiothreitol at 37°C at 150 rpm for 20 min. The epithelial cell layer was removed by intensive shaking, washed and stored for further use. After washing in 10 mL of HBSS with 5 mM EDTA, 1 mM sodium pyruvate and 25 mM HEPES, small intestine pieces were minced with scissors and digested in serum-free media containing 1 mg/mL Collagenase (Millipore Sigma), 0.1 U/mL Dispase (Worthington Biochem, Lakewood, New Jersey) and 0.1 mg/mL DNase I (Millipore Sigma) at 37°C at 150 rpm for 30 min. Cells were washed and passed through a 70 mm cell strainer. Cells were resuspended in 4 mL of 40% Percoll and placed on 4 mL of 80% Percoll. Percoll gradient separation was performed by centrifugation for 20 min at 600 g at room temperature without brake. Lymphoid fractions were collected at the interphase of the Percoll gradient, washed once and resuspended in fluorescence-activated cell sorter buffer or culture medium.
Cells were pelleted, blocked with antimouse CD16/32 (1:500, clone 93; 14-0161-85, eBioscience) and stained with CD3-FITC (1:400, 145–2 C11, eBioscience). Intracellular cytokine staining was performed using RORγt-PE (1:200, B2D, eBioscience) and IL-22-APC (1:100, IL22JOP, eBioscience) antibodies. Intracellular staining was done using the Foxp3/Transcription factor staining buffer set (eBioscience). Cells were recorded using a FACSCanto II flow cytometer. Live single cells were gated using forward scatter and side scatter, and innate immune cells were identified as T cells (CD3+) or innate lymphoid cells (CD3−RORγt+) in which IL-22 expression was assessed. Recorded data were analysed with FlowJo V.10 (Treestar).
Small intestinal contents were collected by squeezing out the contents using sterile forceps and snap-frozen in liquid nitrogen for storage. Indole derivatives were quantified HPLC-coupled to high resolution mass spectrometry as described before.46
Engineered L. reuteri strain
Plasmid pVPL3524 contains a fusion of a synthetic promoter (PRBS1-SP) and the coding sequence of the murine IL-22 gene (NCBI genome accession no. AC153856.23), the latter codon optimised for expression in L. reuteri. Using standard cloning techniques, we replaced the synthetic promoter PRBS1-SP with the L. reuteri EF-Tu promoter to yield plasmid pVPL31126. Plasmid pVPL31126 was transformed in L. reuteri ATCC PTA 6475 by electroporation to yield L. reuteri/IL-22 (Laura M. Alexander, Jan Peter van Pijkeren, manuscript in preparation). As control, we transformed L. reuteri with pJP028, which is the empty vector control that lacks the gene encoding murine IL-22. To test whether L. reuteri/IL-22 colonises following 10 days treatment, faecal samples were collected and cultured overnight at 37 degrees on MRS Broth agar plates.
All data are displayed as mean±SEM. For comparison of two groups, the Student’s unpaired t-test was used. For comparison of >2 groups, one-way analysis of variance was used followed by Tukey’s or Fisher’s least significant difference test. All analyses were performed with GraphPad Prism V.7.03. A p value of <0.05 was considered significant.
Contributors TH designed and performed the experiments, analysed and interpreted the data and wrote the manuscript; YD and YW provided technical support and critically revised the manuscript. J-HO, LMA, PS, SBH, BG, OF, HS and J-PvP provided technical and material support and critically revised the manuscript. BS conceived, designed and supervised the study, wrote and critically revised the manuscript.
Funding This work was supported by an Erwin Schrodinger Fellowship (J4063-B30) from the Austrian Science Fund (to TH), by NIH grants R01 AA020703, R01 AA24726, U01 AA021856 and U01 AA026939 (to BS), R01 GM124494 (to WH) and by Award Number I01BX002213 from the Biomedical Laboratory Research & Development Service of the VA Office of Research and Development (to BS). HS received funding from the European Research Council (ERC) under the European Union’s Horizon 2020 Research and Innovation Programme (ERC-2016-StG-71577). J-PvP was supported by Award Number 233PRJ75PW from the UW-Madison Food Research Institute and by funds from the UW-Madison Institute of Clinical and Translational Research funded by the National Center for Advancing Translational Science award UL1TR000427.
Competing interests None declared.
Patient consent Obtained.
Ethics approval All animal studies were reviewed and approved by the Institutional Animal Care and Use Committee of the University of California, San Diego. For human samples, the protocol was approved by the Ethics Committee of each participating center and patients were enrolled after written informed consent was obtained from each patient.
Provenance and peer review Not commissioned; externally peer reviewed.
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