Non-alcoholic fatty liver disease (NAFLD) is predominantly regarded as a hepatic manifestation of the metabolic syndrome. Approximately, 10–20 % of NAFLD cases develop non-alcoholic steatohepatitis (NASH)(Reference Hyysalo, Mannisto and Zhou1), and 10–15 % of NASH cases progress to cirrhosis, which dramatically increases the incidence of hepatocellular carcinoma(Reference Ratziu, Goodman and Sanyal2). The natural history of NAFLD associated with the high incidence of obesity and type 2 diabetes makes NAFLD the most common cause of chronic liver disease in Western countries and it is predicted to become also the most frequent indication for liver transplantation by 2030(Reference Byrne and Targher3). In the last 10 years, the evidence that NAFLD actively contributes to aggravation of CVD, type 2 diabetes and chronic kidney disease became more and more robust. Therefore, a strong consensus was raised among medical doctors and researchers to consider NAFLD as a multisystem disease(Reference Byrne and Targher3). Thus, NAFLD is a worldwide health concern and medical and dietary strategies to manage and/or prevent its burden are urgent.
The aetiopathology of NAFLD involves many pathways that can be ascribed to the gut–liver axis and that regulate hepatic lipid accumulation and inflammation through the systemic metabolism, gut hormone release and the immune response. Digestion and absorption of dietary nutrients (mainly lipids and glucose), their utilisation and accumulation in the liver and in other tissues (as adipose tissue), glucose uptake and insulin sensitivity, gut microbiota composition, microbial metabolites (such as SCFA or secondary bile acids), as well as inflammatory and gut permeability status are all factors finely associated with the modulation of liver and gut health (for a detailed description of these factors, see the review by Marra & Svegliati-Baroni(Reference Marra and Svegliati-Baroni4)).
The discovery of risk factors and mechanisms underpinning NAFLD development and progression provides biological plausibility to the epidemiological evidence showing negative association between consumption of foods and beverages rich in bioactive compounds with antioxidant and anti-inflammatory capacity (including phytochemicals and dietary fibres) and the risk of liver diseases(Reference Bae, Park and Lee5).
Coffee is one of the most commonly consumed beverages worldwide(Reference Samoggia and Riedel6) and epidemiological evidence shows that its consumption is protective towards several diseases including liver fibrosis, cirrhosis, chronic liver disease and liver cancer(Reference Poole, Kennedy and Roderick7). Noteworthy, inverse associations between coffee consumption and markers of liver disease risk, such as serum levels of liver enzymes, were reported for both caffeinated and decaffeinated coffee by Xiao et al. (Reference Xiao, Sinha and Graubard8), while the lack of significant associations for decaffeinated coffee in the analysis of Dickson et al. (Reference Dickson, Liese and Lorenzo9) could be explained by the generally modest consumption of that type of coffee and narrow range of intakes in the population. Similarly, the recent meta-analysis by Kennedy et al. (Reference Kennedy, Roderick and Buchanan10), including data from the few studies that specified coffee type consumed by population, showed that the increase of caffeinated and decaffeinated coffee consumption by two cups per d reduced the risk of hepatocellular carcinoma by 27 and 14 %, respectively. These observations are in line with scientific literature showing that components in coffee other than caffeine may be critical in eliciting the health benefits of the beverage (for reviews on coffee bioactive components and mechanisms underpinning benefits, see Salomone et al. (Reference Salomone, Galvano and Li Volti11), Assy et al. (Reference Assy, Nasser and Kamayse12) and Alferink et al. (Reference Alferink, Kiefte-de Jong and Darwish Murad13)).
Among coffee components, particular attention has been devoted to polyphenols and melanoidins. They are considered the coffee components with the highest chances of eliciting health benefits, and also against colorectal cancer, because they can arrive, in part, at the colon, thus interacting with local microbiota(Reference Vitaglione, Fogliano and Pellegrini14). Current trends in personalised nutrition point to the microbiota as one of the principal targets to modulate health(Reference De Filippis, Vitaglione and Cuomo15), but it is still underinvestigated in research focused on the health effect of coffee.
We previously investigated the individual roles of coffee polyphenols and melanoidins on antioxidant and anti-inflammatory effects in the liver and blood of an animal model of NAFLD(Reference Vitaglione, Morisco and Mazzone16). Data demonstrated that whole coffee was more effective than separated fractions to protect the liver from high-fat diet (HFD)-induced damage through a reduction in hepatic fat accumulation, systemic and liver oxidative stress and inflammation(Reference Vitaglione, Morisco and Mazzone16).
The scientific literature indicates that gut health is implicated in the development and progression of liver diseases and very little recent evidence exists that coffee can modulate some intestinal functions(Reference Brandt, Nier and Jin17).
The present study aimed at clarifying the effect of coffee consumption on gut pathways implicated in NAFLD development such as intestinal and liver lipid metabolism, gut barrier functions and gut microbiota. To this purpose an animal study with mice fed an HFD and drinking water or a coffee extract as well as mice fed with a standard diet (SD) and drinking water for 12 weeks was implemented. Serum samples and liver histology were assessed in parallel with gene expression of molecular mediators of fat oxidation, cholesterol efflux, lipid digestion and energy metabolism regulation, gut permeability and composition of the gut microbiota.
Materials and methods
Animals and treatments
A sample size calculation, based on variations from a previous study(Reference Matsuda, Kobayashi and Yamauchi18), showed that eight animals per treatment group would be sufficient to detect a threefold decrease in alanine aminotransferase (ALT) serum concentration with an α error of 0·05, a statistical power of 0·8 and two-sided testing in coffee-treated v. control mice.
A total of twenty-four male C57BL/6J mice, 4 weeks old, weighing 20 ± 0·5 g were housed randomly in wire-bottomed cages. Animals were obtained from Harlan Italy and were maintained under controlled temperature conditions of 22 ± 1°C, with a 12 h light–dark cycle and free access to water.
Mice were divided into three groups (n 8 each) and assigned to one of the following 12-week diets: (1) SD; (2) HFD; (3) HFD plus decaffeinated coffee solution (HFD+COFFEE).
The SD was a low-glycaemic control diet (TD.120455; Envigo Teklad). It contained 186 g/kg of proteins (19 % of energy), 506 g/kg of carbohydrates (51 % of energy), 62 g/kg of fat (6 % of energy), 35 g/kg of cellulose and provided 3·3 kcal/g (13·8 kJ/g).
The HFD was an adjusted-energy diet (TD.06414; Envigo Teklad). It contained 235 g/kg of protein (18 % of energy), 273 g/kg of carbohydrates (21 % of energy), 343 g/kg of fat (60 % of energy), 65·5 g/kg of cellulose and provided 5·1 kcal/g (21·3 kJ/g).
A detailed composition of the two diets is reported in Supplementary Table S1.
Coffee-containing beverages were prepared by filtering on a filter paper (Whatman grade 113; Merck KGaA), a mix of boiling water and decaffeinated coffee powder (4:1, v/w) (Illy Caffè). Filtered coffee was portioned and stored at −20°C until used. In a preliminary experiment, we found that the average daily consumption of solution (water or the coffee solution) was about 3·5 (sd 0·3) ml/mouse/d. The coffee-based beverage was prepared by diluting 1·5 ml of coffee in 100 ml of water.
The dose of administered coffee corresponded to six cups of espresso coffee or two cups of filtered coffee for a person weighing 70 kg. Food and energy intake as well as body weight were recorded weekly. Food intake was calculated based on the amount of food remaining from a known amount administered weekly.
At baseline, and at 2, 6 and 10 weeks of intervention, stool samples were collected, were snap-frozen in liquid N2 and stored at −80°C until DNA extraction was performed.
After 12 weeks of treatment, animals fasting for 12 h were killed by using a lethal dose of anaesthetic and the liver, duodenum, colon and caecum with all the contents were harvested and snap-frozen until analyses. A portion of liver tissues was fixed in 4 % formaldehyde and embedded in paraffin.
The experimental protocol was approved by the Ethics Committee for animal experiments at the Federico II University of Naples according to the institutional guidelines. All animals received humane care according to the criteria outlined in the National Institutes of Health Guide for the Care and Use of Laboratory Animals (National Institutes of Health Publication, eighth edition, 2011).
Sections (5 μm thick) were obtained and stained with haematoxylin and eosin. A liver pathologist, who was blind to the intervention, performed the histological analysis, by evaluating the whole sections. Macrovesicular steatosis was assessed at low magnification (4×) as percentage of affected hepatocyte and scored as grade 0 (between 0 and 5 %), grade 1 (between 6 and 33 %), grade 2 (between 34 and 66 %) and grade 3 (>66 %). Microvesicular steatosis was also evaluated at higher magnification (20×) and recorded as percentage of affected cells. Necro-inflammatory lobular foci were sought and scored as present or absent.
Biochemical analyses of serum samples
Serum ALT, total cholesterol and TAG were measured using the routinely automatised assays (Reflotron Plus system from Roche Diagnostic). Liver TAG content was measured in lipid extracts from previously frozen liver tissue using a TAG quantification kit (BioVision) according to the manufacturer's protocol. Data obtained were normalised by tissue protein concentration measured by the Bradford assay (Bio-Rad).
Analysis of liver and intestinal specimens
Gene expression of PPAR- α, acyl-CoA oxidase 1 (ACOX1), ATP-binding cassette (ABC) subfamily A1 (ABCA1) and liver X receptor-α (LXR-α) in liver samples, of peptide YY (PYY), free fatty acid receptor-1 (FFAR-1), FFAR-3, claudin, occludin, zonulin-1 (ZO-1), ABCA1 and ABC subfamily G1 (ABCG1) in duodenum samples and of FFAR-1, FFAR-3 and ZO-1 in colon samples was evaluated by quantitative real-time (RT)-PCR analysis. Total RNA was extracted using an RNeasy Plus Mini Kit (Qiagen) from liver, duodenum and colon biopsies. The purity of total RNA was assessed using a NanoDrop ND-100 spectrophotometer at 260 nm. A quantity of 2 μg of total RNA was used in the first-strand cDNA synthesis by TaqMan Reverse Transcription Reagents (Applied Biosystems). The cDNA was diluted with RNase-free water for a final volume of 200 ml and stored at −20°C until used. PPAR- α, ACOX1, PYY, FFAR-1, FFAR-3, claudin, occludin, ZO-1, ABCA1, ABCG1 and LXR- α gene expression levels were analysed by Taq-Man Gene Expression Assays (Applied Biosystems) (Supplementary Table S2). Quantitative RT-PCR was carried out in triplicate using a pre-optimised primer/probe mixture and TaqMan Universal PCR Master Mix (Applied Biosystems) on a StepOne™ RT-PCR system in a forty-eight-well format (Applied Biosystems). The glyceraldehyde 3-phosphate dehydrogenase (GAPDH) housekeeping gene was used as an endogenous control, for normalisation of gene expression assays. The relative gene expression data were assessed by using the ΔΔCt method. The sample values represent X-fold differences from a control sample (given a designated value of 1) within the same experiment.
Lipid composition of caecal content
Extraction of lipids from caecal content samples was performed according to Gregory et al. (Reference Gregory, Bird and Gross19) with brief modifications. The extracts were analysed by liquid chomatography-high resolution MS by briefly adapting the method described by Bird et al. (Reference Bird, Marur and Sniatynski20). Data were acquired on an Accela U-HPLC system coupled to an Exactive Orbitrap mass spectrometer (Thermo Fisher Scientific) equipped with a heated electrospray interface. A Kinetex 2·6 µ C18 100 A column (100 × 2·1 mm) (Phenomenex) thermostated at 45°C was used. The mobile phases consisted of 40:60 water–acetonitrile, 5 mm-ammonium formate and 0·1 % formic acid (A) and 90:10 isopropanol–acetonitrile, 5 mm-ammonium formate and 0·1 % formic acid (B). A gradient elution as in Vitaglione et al. (Reference Vitaglione, Fogliano and Pellegrini14) was applied. The flow rate was set at 200 µl/min and the injection volume was 10 µl. Acquisition was performed in both positive and negative ionisation modes, in the mass range of m/z 120–1200. The resolving power was set to 50 000 full width at half-maximum (m/z 200) resulting in a scan time of 1 s. The automatic gain control was used in balanced mode (1 × 106 ions); maximum injection time was 100 ms. The interface parameters were as follows: spray voltage was at 3·5 kV (positive mode) and 3·0 kV (negative mode), capillary voltage 30 V, heater temperature at 350°C, capillary temperature at 250°C, sheath gas at 35 arbitrary units, and auxiliary gas at 15 arbitrary units. Chromatographic data acquisition and peak integration were performed using Xcalibur software (Thermo Fisher Scientific).
NEFA identification was obtained using ExactFinder 2.0 software (Thermo Fisher Scientific) by the application of a homemade database. Specific molecular formulas and their respective m/z ratios were included in ExactFinder and the following parameters were selected: exact mass of monoisotopic ion (experimental mass tolerance accuracy less than 5 parts per million), isotopic pattern, retention time, signal:noise ratio higher than 5.
TAG were detected in positive mode as predominately (M + NH4)+ ions and were integrated in the chromatographic region between retention times of 22–24·5 min. NEFA were detected in negative mode as (M − H)− ions in the chromatographic region between 3 and 7·5 min.
Gut microbiota composition
Faecal samples (about 0·3 g) were used for DNA extraction with the PowerSoil DNA Isolation kit (Mo Bio Laboratories, Inc.). The V1–V3 region of the 16S rRNA gene (about 520 bp) was amplified and PCR libraries were prepared and sequenced as previously reported(Reference De Filippis, Pellegrini and Vannini21).
The sequences were analysed and filtered using QIIME 1.9.0 software(Reference Caporaso, Kuczynski and Stombaugh22). Quality filtering, de novo operational taxonomic unit (OTU) picking and taxonomy assignment were carried out as previously described(Reference De Filippis, Vannini and La Storia23). To avoid biases due to the different sequencing depths, OTU tables were rarefied to the lowest number of sequences per sample.
The 16S rRNA gene sequences produced in this study are available at the Sequence Read Archive (SRA) of the National Center for Biotechnology Information (NCBI), under accession number PRJNA434511.
All the animals (eight per group) were included in each analysis. Data are reported as means with their standard errors. Groups were compared using ANOVA followed by Tukey's multiple-comparison tests. A P value of less than 0·05 was considered statistically significant.
For the faecal microbiota composition statistical analyses were carried out using R (https://www.r-project.org). Differential abundance of specific taxa according to diet or coffee assumption was determined by DeSeq2(Reference Love, Huber and Anders24). Principal components analysis was carried out on the normalised abundance (log10) of the microbiota at genus level (dudi.pca function in the R package made4). Permutational multivariate ANOVA (non-parametric MANOVA) based on Jaccard distance matrix was carried out by using 999 permutations to detect significant differences in the overall bacterial community composition as affected by the type of diet or coffee consumption, by using the adonis function in the vegan package.
Body weight and food intake
After 12 weeks, HFD-fed mice (with or without coffee) weighed significantly more than mice fed the SD (P < 0·001 for both groups) (Supplementary Fig. S1). Starting from week 8, HFD- and HFD+COFFEE-fed mice had different growth curves. HFD+COFFEE-fed mice gained progressively less body weight compared with HFD-fed mice (P < 0·05). This difference was maintained until week 12 when HFD+COFFEE-fed mice weighed 34·8 (se 2·5) g and HFD-fed mice weighed 38·4 (se 3·0) g (P < 0·01). Food intake data showed that HFD- and HFD+COFFEE-fed mice had higher energy intake than SD-fed animals (386·2 (se 7·1) and 369·2 (se 5·8) v. 253·0 (se 2·6) kcal (1615·9 (se 29·7) and 1544·7 (se 24·3) v. 1058·6 (se 10·9) kJ); P < 0·001 for both comparisons). Moreover, HFD+COFFEE-fed mice had higher food intake than HFD-fed mice (386·2 (se 7·1) v. 369·2 (se 5·8) kcal (1615·9 (se 29·7) v. 1544·7 (se 24·3) kJ); P < 0·05) (Supplementary Fig. S1(B)).
As concerns liver weight, data showed a reduced liver:body weight ratio in HFD+COFFEE-fed mice compared with HFD-fed mice (3·06 (se 0·06) v. 3·47 (se 0·15); P < 0·05) and SD-fed mice (3·06 (se 0·06) v. 3·59 (se 0·06); P < 0·01).
Serum parameters and liver steatosis
Serum total cholesterol, TAG, ALT and glycaemia are reported in Table 1. Both groups of HFD-fed mice had higher circulating concentrations of total cholesterol than SD-fed mice (P < 0·0001 for HFD and P = 0·0097 for HFD+COFFEE v. SD). However, lower concentrations were recorded in HFD+COFFEE-fed than HFD-fed mice (P = 0·0001). Similarly, coffee intake reduced serum ALT in HFD-fed mice (P = 0·0280). Interestingly, a significant reduction in blood glucose in HFD+COFFEE- v. SD-fed mice (P = 0·0085) was also observed.
SD, standard diet; HFD, high-fat diet; HFD+COFFEE, HFD plus decaffeinated coffee.
** Mean value was significantly different from that for the SD-fed mice (P < 0·001; ANOVA and Tukey's post hoc analysis).
Mean value was significantly different from that for the HFD-fed mice: † P < 0·05, †† P < 0·001 (ANOVA and Tukey's post hoc analysis).
‡ To convert cholesterol in mg/dl to mmol/l, multiply by 0·0259. To convert TAG in mg/dl to mmol/l, multiply by 0·0113. To convert glucose in mg/dl to mmol/l, multiply by 0·0555.
Coffee consumption caused a reduction in liver steatosis induced by the HFD. Macrovesicular steatosis was scored 0 in all livers from SD- and HFD+COFFEE-fed mice, whereas in the HFD group only three cases had a score of 0. The difference in steatosis grade between the HFD and SD and HFD+COFFEE groups was significant (P < 0·01) (Supplementary Fig. S2). Microvesicular steatosis was also less severe in HFD+COFFEE- than HFD-fed mice, even if the difference between the two groups was not statistically significant. Necro-inflammatory lobular foci were seen in four of the HFD-fed mice and none of the HFD+COFFEE-fed group (P = 0·01) (Fig. 1).
Liver factors underpinning fat deposition
Fig. 2 shows the gene expression of liver PPAR-α and ACOX1 of mice in the three groups. Data showed a threefold and twofold up-regulation of PPAR-α and ACOX1 mRNA expression, respectively, in the liver of HFD+COFFEE-fed mice compared with SD-fed animals (P = 0·0228 and P = 0·0103) and with HFD-fed mice (P = 0·0160 and P = 0·0355). This suggested that coffee can promote β-oxidation in the liver.
Liver and intestinal factors underpinning cholesterol efflux
Fig. 3 shows the effect of treatments on gene expression of hepatic LXR-α (Fig. 3(A)) and ABCA1 (Fig. 3(B)) as well as duodenal ABCA1 (Fig. 3(C)) and ABCG1 (Fig. 3(D)). Liver LXR-α mRNA expression was increased by coffee consumption, while liver ABCA1 mRNA expression appeared slightly increased following the HFD compared with the SD but the difference did not reach statistical significance (P = 0·07). On the other hand, at intestinal level, an up-regulation of both ABCA1 and ABCG1 gene expression in HFD+COFFEE-fed v. HFD-fed mice (P = 0·0164 and P = 0·0306) was found; however, although the mRNA expressions were slightly increased v. SD-fed mice, they were not significant (P = 0·0882 and P = 0·0895). These findings suggested that coffee intake can stimulate cholesterol efflux.
Intestinal factors implicated in lipid sensing and energy metabolism
Fig. 4 shows the effect of treatments on gene expression of duodenal and colonic FFAR-1 (Fig. 4(A) and (B)) and FFAR-3 (Fig. 4(C) and (D)) as well as duodenal PYY (Fig. 4(E)). Coffee consumption up-regulated FFAR-1 in both duodenum (P = 0·021 v. HFD and P = 0·029 v. SD) and colon tissue (P = 0·031 v. HFD and P = 0·043 v. SD) whereas FFAR-3 in the colon was up-regulated by the HFD independently from coffee (P = 0·005 for HFD v. SD and P = 0·012 for HFD+COFFEE v. SD). PYY gene expression was up-regulated in the duodenum of HFD+COFFEE- v. SD-fed mice (P < 0·01) while no differences were recorded between HFD+COFFEE- and HFD-fed mice or HFD- and SD-fed mice.
Interestingly, the analysis of lipids in the caecum content showed that HFD+COFFEE-fed mice had 2·2 and 2·5 times higher amount of total lipids in the caecum than HFD- and SD-fed mice, respectively. Furthermore, looking at lipid composition, HFD+COFFEE-fed mice showed a NEFA:TAG ratio that was ten times lower than HFD-fed mice (0·02 v. 0·16 %), thus meaning that the lipids were mainly in the form of TAG (Supplementary Fig. S3).
Intestinal permeability and gut microbiota
To establish whether coffee consumption may modulate intestinal permeability, the gene expression of the tight junctions ZO-1, occludin and claudin on intestinal specimens was assessed (Fig. 5). Significant up-regulations of duodenal and colonic ZO-1 and duodenal claudin mRNA expression with the HFD+COFFEE v. HFD (P = 0·035, P = 0·044 and P = 0·016, respectively) and v. the SD (P = 0·020) were found.
Conversely, occludin gene expression was down-regulated by the HFD and HFD+COFFEE v. the SD (P = 0·0027 and P = 0·0006, respectively).
Faecal microbiota was strongly affected by the type of diet (HFD v. SD) (P < 0·05). In particular, levels of Alistipes, Odoribacter and Allobaculum increased while Muribaculum was reduced with the HFD compared with the SD (P < 0·05) (Fig. 6). Interestingly, coffee intake was associated with a significant increase in Alcaligenaceae in HFD-fed mice (0·33 % in HFD+COFFEE v. 0·03 % in HFD), regardless of the length of the treatment. Principal components analysis showed a clear clustering of the samples according to diet (Supplementary Fig. S4(A)). Nevertheless, when the analysis was carried out on HFD- or SD-fed mice separately, an effect of coffee intake was observed. Samples after 6 and 10 weeks of coffee consumption (HFD+COFFEE; Supplementary Fig. S4(B)) separated from the HFD. This separation was mainly driven by the different abundance of Alistipes, Bacteroides and Odoribacter.
In this study, the molecular mechanisms underpinning the effects of coffee on NAFLD induced by an HFD were elucidated by focusing on pathophysiological pathways linking the gut and liver. The main findings are summarised in Fig. 7.
Coffee consumption reduced HFD-induced liver steatosis and circulating ALT, which is consistent with our previous findings(Reference Vitaglione, Morisco and Mazzone16). The reduced fat deposition (as demonstrated by histopathology and supported by the reduced liver:body weight ratio) and inflammation in the liver could be a consequence of an increased fat oxidation(Reference Souza-Mello25), which was supported by the up-regulation of PPAR-α. This is in agreement with other studies demonstrating the ability of polyphenols, as pure compounds or as part of foods, to induce lipid oxidation in the liver of animals fed with an HFD(Reference Salomone, Godos and Zelber-Sagi26). The hypothesis of coffee-induced fat oxidation in the liver is further supported, in the present study, by the up-regulation of ACOX1. Indeed, ACOX1 is responsible for the second reaction of peroxisomal β-oxidation(Reference Reddy and Hashimoto27) and its up-regulation together with PPAR-α was a key factor in the hypolipidaemic effect of a polyphenol-rich walnut extract(Reference Shimoda, Tanaka and Kikuchi28) as well as of an apple peel extract and quercetin in HFD-fed mice(Reference Snyder, Zhao and Luo29).
Differently from our previous study in rats(Reference Vitaglione, Morisco and Mazzone16) coffee did not modulate serum TAG but reduced blood cholesterol and glucose in the present study. Both effects are possibly mediated by liver LXR-α whose activation is in line with that of PPARα(Reference Li and Glass30). LXR-α could regulate systemic cholesterol homoeostasis by increasing biliary cholesterol excretion through regulation of the intestinal membrane transporters ABCA1 and ABCG1(Reference Boullier, Bird and Chang31). Indeed, the two transporters act synergistically to remove cholesterol from cells: ABCA1 converts lipid-poor apoA-I to partially lipidated ‘nascent’ lipoproteins which are effective acceptors for cholesterol exported through the basolateral membrane by ABCG1(Reference Vaughan and Oram32). On the other hand, activation of LXR-α could also modulate liver gluconeogenesis and adipose tissue insulin-sensitive glucose transporter (GLUT4) by inducing glucose utilisation in the liver and storage in adipocytes(Reference Laffitte, Chao and Li33). At the intestinal level, the up-regulation of gene expression of the long-chain fatty acids receptor FFAR-1 could further support the ameliorated glucose metabolism in coffee- compared with water-drinking mice. FFAR-1 activation by NEFA in the intestinal lumen induces the secretion of glucagon-like peptide-1 and glucose-dependent insulinotropic polypeptide, which can stimulate insulin secretion glucose-dependently, thus possibly contributing to the hypoglycaemic effect elicited by coffee in HFD-fed mice(Reference Edfalk, Steneberg and Edlund34). Moreover, FFAR-1 activation elicits cholecystokinin response that, in turn, can stimulate secretion of pancreatic lipase and fat absorption(Reference Lo, King and Samuelson35). Therefore, it was hypothesised that FFAR-1 up-regulation was an intestinal adaptive mechanism to compensate for the lacking fat digestion caused by the inhibitory activity of coffee polyphenols on pancreatic lipase(Reference Cha, Song and Kim36–Reference Almoosawi, McDougall and Fyfe38). Indeed, lipid characterisation of caecum contents showed that the NEFA:TAG ratio was lower in HFD+COFFEE-fed mice than HFD-fed mice. An ameliorated fat absorption consequent to FFAR-1 up-regulation and possibly induced by a reinforced cholecystokinin response might provide an explanation for the similar TAG serum level in HFD- and HFD+COFFEE-fed mice despite the latter showing a reduced fat digestion.
Although statistical significance was not reached, coffee consumption slightly increased the gene expression of duodenal PYY in HFD+COFFEE-fed mice. This observation goes in parallel with a higher food intake but lower body weight gain for HFD+COFFEE- v. HFD-fed mice. We hypothesised that possibly higher levels of PYY in these mice failed to increase satiety because in the presence of lipase inhibitors from coffee an attenuation of the inhibitory effect of oral fat on food intake might have occurred(Reference O'Donovan, Feinle-Bisset and Wishart39). On the other hand, the lower body weight of coffee-drinking mice than the others lets us hypothesise that higher levels of PYY might have boosted energy expenditure and fat oxidation rate in HFD+COFFEE-fed mice(Reference Guo, Ma and Enriori40).
Another important finding of the present study is that coffee might have ameliorated gut permeability as suggested by the restoration of zonulin-1 gene expression in the duodenum and colon as well as claudin in the duodenum of HFD+COFFEE-fed mice v. HFD-fed mice. An improved gut barrier function induced by coffee in the present study could explain the reduced liver steatosis and the lower serum levels of cholesterol and glucose. Moreover, it is in agreement with our previous observation in rats(Reference Mazzone, Lembo and D'Argenio41) and with the recent findings of Brandt et al. (Reference Brandt, Nier and Jin17) who found that consumption of decaffeinated coffee in mice fed with a high-fat, -fructose and -cholesterol diet increased intestinal protein expression of zonulin-1 and occludin, reduced bacterial endotoxin concentration in portal blood and mRNA expression of lipopolysaccharide-binding protein in the liver compared with the mice fed with the same diet without coffee. It is well known that HFD is associated with dysbiosis, intestinal mucosa inflammation and a leaky gut condition leading to metabolic endotoxaemia and consequent liver fat accumulation and inflammation(Reference Cani, Bibiloni and Knauf42). Prebiotics, such as inulin-type fructans, were shown to revert those conditions by modulating gut microbiota(Reference Tilg, Cani and Mayer43–Reference Cani, Possemiers and Van de Wiele45). However, in the present study the overall structure of the gut microbiota was not significantly changed by coffee consumption, as determined by MANOVA. Nevertheless, increased abundance of Alcaligenaceae was found in mice fed the HFD and drinking coffee. Alcaligenaceae were shown to metabolise oestradiol in vitro (Reference Payne and Talalay46) and were negatively associated with the total cholesterol concentration in a population with atherosclerosis(Reference Ziganshina, Sharifullina and Lozhkin47). Therefore, it can be speculated that these bacteria might be implicated in the intestinal re-absorption of cholesterol, thus providing an upstream mechanism of cholesterol efflux to the effect of coffee on lowering serum cholesterol in the present study. A high abundance of Alcaligenaceae was also observed by Zhou et al. (Reference Zhou, Hergert and Rompato48) in mice supplemented with whole grain oat (WGO) flour and experiencing a lower blood cholesterol and improvement of insulin sensitivity in comparison with the mice supplemented with low bran oat (LBO) flour. The similar findings between the present study and the study by Zhou et al. (Reference Zhou, Hergert and Rompato48) could be related to the feature of WGO and coffee to be sources of antioxidant dietary fibres. Indeed, the WGO diet contained a 1·4 % (w/w) more soluble fibre (mainly β-glucans) and specific phytochemicals including phenolic acids, alkyl- and alkenylresorcinols, and avenanthramides compared with LBO. Coffee used in the present study contained melanoidins and polyphenols. Melanoidins are known to behave physiologically as dietary fibre, i.e. they can arrive undigested to the colon and can be fermented by local microbiota(Reference Morales, Somoza and Fogliano49). In addition, since melanoidins entrap polyphenols in their structure, they are chemically similar to the antioxidant cereal dietary fibres and, similarly, they behave as natural carriers of polyphenols to the colon, thus possibly beneficing colon health and nutrient metabolism through the modulation of the gut microbiota composition and functions(Reference Vitaglione, Fogliano and Pellegrini14, Reference Vitaglione, Napolitano and Fogliano50).
Altogether, the mechanisms showed in our study support epidemiological data demonstrating that coffee reduces the prevalence and incidence of the metabolic syndrome(Reference Marventano, Salomone and Godos51).
In conclusion, we provided first evidence that coffee consumption reduces HFD-induced liver damage by modulating pathways involved in the gut–liver axis.
Coffee reduced the HFD-induced liver steatosis and metabolic derangement by:
Reducing hepatic fat deposition possibly through increased fat oxidation in the liver;
Increasing cholesterol intestinal efflux;
Reducing lipid digestion and ameliorating the intestinal system involved in lipid sensing and energy metabolism regulation, and
Ameliorating gut barrier function through a restoration of tight junction proteins in the duodenum and colon.
All these mechanisms were accompanied by a negligible change in gut microbiota composition.
The supplementary material for this article can be found at https://doi.org/10.1017/jns.2019.10
There are no acknowledgments.
Experiments were conducted with departmental funding. The funding source had no involvement in decisions related to the research and publication of results.
N. C., F. M. and P. V. designed the experiments, G. M., V. L., G. D. and A. R. carried out the experiments and managed animals; G. M. and M. S. performed biological analyses; M. G. and F. S. performed histology; I. M. and P. V. performed analysis of lipids; F. D. F. and D. E. performed analysis of gut microbiota; P. V., G. M. and N. C. wrote the article; P. V., N. C. and F. M. had primary responsibility for final content. All authors read and approved the final manuscript.
There were no conflicts of interest.