Naringenin (4′,5,7-trihydroxyflavanone), one of the most abundant flavonoids in citrus, grapefruits and tomatoes, has been reported to exhibit interesting pharmacological activities, such as anti-oxidation, anti-inflammation and anti-tumour(Reference Park, Kim and Choi1, Reference Yadav, Prasad and Sung2). A recent investigation suggested that naringenin co-administration significantly ameliorated the extent of intestine oedema in a mice model of dextran sulphate sodium (DSS)-induced colitis(Reference Maria Inês Amaro, João Rocha and Helder Vila-Real3); however, the underlying mechanism has not yet been investigated.
The molecular signalling pathways governing intestinal inflammation are varied; however, a distinct pathway of inflammation comes from signals originating from the interaction of the gut commensal bacteria and the host mucosa(Reference Cucchiara, Stronati and Aloi4, Reference Neurath and Travis5). Indeed, the exact nature of these signals, as to one that initiates host inflammation, remains debated. It is clear that invariably there is dysbiosis in gut inflammatory diseases (e.g. inflammatory bowel disease (IBD))(Reference Mazmanian, Round and Kasper6), and along with dysbiosis, there is dysregulation of pattern-recognition receptors that recognise pathogen-associated molecular patterns(Reference Saunders, Barlow and Walsh7). Together, these are essential triggers of release of pro-inflammatory cytokines in the gut, which has paved the path towards discovery of pharmacological targets of IBD(Reference Levin and Shibolet8–Reference Fukata and Abreu10). One such pattern-recognition receptor, Toll-like receptor 4 (TLR4), a key receptor for commensal recognition in gut innate immunity, is over-expressed in inflamed colonocytes and is the subject of therapeutics (target inhibition) in IBD(Reference Ungaro, Fukata and Hsu11, Reference Heimesaat, Fischer and Jahn12). As one of the innate immune receptors, TLR4 signals through recruitment of the adaptor proteins myeloid differentiation primary response gene 88 (MyD88) and Toll/interleukin 1 receptor domain-containing adaptor protein inducing IFN-β (TRIF)(Reference Núñez Miguel, Wong and Westoll13). MyD88 signalling results in NF-κB activation, while TRIF signalling activates both NF-κB and interferon-regulatory factor 3. Thereby, TLR4-induced signalling leads to activation of NF-κB and interferon-regulatory factor 3, followed by a pleiotropic gene expression involved in immune and inflammatory responses(Reference Lin, Yin and Zhong14). Thus, it is proposed that many therapeutic targets that abrogate intestinal inflammation might transect with the TLR4 signalling pathway(Reference Ungaro, Fukata and Hsu11, Reference Fiorotto, Scirpo and Trauner15). Based on the key role that TLR4 plays in enterocyte inflammation, we investigated the role of naringenin in inhibiting TLR4-linked NF-κB signalling pathway in DSS-induced murine colitis.
Materials and methods
Materials and animals
Naringenin (molecular weight 272·25 Da, HPLC ≥ 98 %) was obtained from the Shanghai R&D Center for Standardization of Traditional Chinese Medicine, Shanghai, China. Mouse macrophage RAW264.7 cells and human colorectal carcinoma HT-29 cells were purchased from the American Type Culture Collection and maintained in a normal state according to the culture manual. For in vivo studies, naringenin stock solution was prepared in 0·5 % (w/v) methylcellulose and administered orally to mice at a dose of 50 mg/kg per d. Naringenin dosing was similar to previous reports(Reference Kannappan, Palanisamy and Anuradha16, Reference Ortiz-Andrade, Sánchez-Salgado and Navarrete-Vázquez17). As vehicle control, all mice received an equivalent volume (compared with experimental groups) of 0·5 % (w/v) methylcellulose solution. Healthy 8- to 10-week-old female C57BL/6 mice (20 (sd 2) g) were obtained from the Laboratory Animal Center of Shanghai University of Traditional Chinese Medicine, and studies were performed in accordance with the guidelines approved by the Animal Ethics Committee of the Shanghai University of Traditional Chinese Medicine, Shanghai. All mice were housed under a specific pathogen-free facility at the Shanghai University of Traditional Chinese Medicine, under the same laboratory conditions of temperature (25 ± 2°C) and lighting (12 h light–12 h dark cycle) and were given free access to standard laboratory chow (containing 10 % fat, 70 % carbohydrates and 20 % protein by energy, supplied by the Shanghai SLAC Experimental Animal Company Limited) and tap water.
Experimental design
Mouse IBD studies were performed as described previously(Reference Dou, Mukherjee and Li18). The experiment lasted for 10 d. Mice were distributed into four groups (n 10–15 mice per group) based on age (8+ and 9+ weeks, for each round of mouse IBD studies. Mouse IBD studies were repeated twice) and body weight (randomly distributed among four groups): group 1, vehicle controls were administered 100 μl of 0·5 % (w/v) methylcellulose orally once per d; group 2, naringenin at a dose of 50 mg/kg of body weight via oral administration once per d; group 3, 100 μl of 0·5 % (w/v) methylcellulose by oral administration once per d and 4 % (w/v) DSS (molecular weight 36 000–50 000 Da; MP Biomedicals) in drinking-water from days 4 to 10; group 4, received naringenin by oral administration (50 mg/kg of body weight) 3 d prior to DSS treatment and continued till the end of DSS treatment. Total volume orally administered was identical for each group.
Colitis evaluation
Mice were monitored daily for signs of body movement, body weight, diarrhoea and bloody stools. Bloody diarrhoea events were evaluated clinically by inspection of anal discharge, and a percentage value was determined based on the number of animals with this condition at any given point of time(Reference Wallace, Wang and Lane19). After killing the mice under anaesthesia, the entire colon was excised and placed on an ice plate and cleaned of fat and mesentery. The length of each colon specimen was measured. The distal and proximal colons were taken and fixed in 10 % (w/v) buffered formalin for 24 h at room temperature and embedded in paraffin and stained with haematoxylin–eosin for histological evaluation. Histological damage was assessed as a combined score of inflammatory cell infiltration (score 0–3) and mucosal damage (score 0–3) using a method previously described(Reference Siegmund, Lehr and Fantuzzi20). For inflammatory cell infiltration in the colon mucosa, rare inflammatory cells (mononuclear infiltrates) in the lamina propria were counted as 0; increased numbers of inflammatory cells, including neutrophils in the lamina propria, as 1; confluence of inflammatory cells, extending into the submucosa as 2; and a score of 3 was given for transmural extension of the inflammatory cell infiltration. For epithelial damage, absence of mucosal damage was counted as 0, discrete focal lymphoepithelial lesions were counted as 1, mucosal erosion/ulceration was counted as 2 and a score of 3 was given for extensive mucosal damage and extension through deeper structures of the bowel wall. The two sub-scores were added and the combined histological score ranged from 0 (no changes) to 6 (extensive cell infiltration and tissue damage).
Western blot analysis
Colon tissues were disrupted by homogenisation on ice and centrifuged at 4°C (12 000 g, 15 min). The supernatants were collected and protein concentrations were determined. Equal amounts of protein (40 μg/lane) were separated on 10 % SDS-PAGE and transferred to nitrocellulose membrane. Membranes were blocked in 5 % (w/v) skimmed milk and incubated with antibodies against mouse TLR4 (sc-293072, 1:1000; Santa Cruz Biotechnology), phospho-p65 (#3033, 1:1000; Cell Signaling Technology, Inc.), phospho-IκBα (#2859, 1:1000; Cell Signaling) and β-actin (#4970, 1:2000; Cell Signaling). Blots were then washed three times with PBS containing 0·1 % (w/v) Tween-20 and incubated with horseradish peroxidase-conjugated secondary antibodies (Santa Cruz). Blots were again washed with PBS containing 0·1 % (w/v) Tween-20, and then developed by enhanced chemiluminescence detection regents (Amersham). The protein bands were quantified by the average ratios of integral optic density following normalisation to the housekeeping gene β-actin expression.
RNA analysis
RNA was extracted from colon tissues using TRIzol reagent (Invitrogen). Quantitative real-time PCR was performed using complementary DNA generated from 3 μg total RNA with the SuperScript II Reverse transcriptase kit (Invitrogen). The primer sequences used in PCR amplification are as follows: 5′-TTCAGAGCCGTTGGTGTATC-3′/5′-CCCATTCCAGGTAGGTGTTT-3′ for TLR4, 5′-GGGAATCTTGGAGCGAGTTG-3′/5′-GTGAGGGCTTGGCTGAGTGA-3′ for inducible NO synthase (iNOS), 5′-CGCTGTGCTTTGAGAACTGT-3′/5′-AGGTCCTTGCCTACTTGCTG-3′ for intercellular adhesion molecule-1 (ICAM-1), 5′-AAGTTGACCCGTAAATCTGA-3′/5′-TGAAAGGGAATACCATAACA-3′ for monocyte chemoattractant protein-1 (MCP-1), 5′-GAAGTCTTTGGTCTGGTGCCT-3′/5′-GCTCCTGCTTGAGTATGTCG-3′ for cyclo-oxygenase-2 (Cox2), ′-CGTGGAACTGGCAGAAGAGG-3′/5′-AGACAGAAGAGCGTGGTGGC-3′ for TNF-α, 5′-ACCACGGCCTTCCCTACTTC-3′/5′-CATTTCCACGATTTCCCAGA-3′ for IL-6, 5′-CAGCCTTCCTTCTTGGGTAT-3′/5′-TGGCATAGAGGTCTTTACGG-3′ for β-actin. PCR were carried out using SYBR Premix ExTaq Mix (Takara Biotechnology) in an ABI Prism 7900HT Sequence Detection System (Applied Biosystems). Thermal cycler parameters were as follows: one cycle of 95°C for 30 s, forty cycles of denaturation (95°C, 5 s) and combined annealing/extension (60°C, 30 s). Gene expression changes were calculated by the comparative C t method and the values were normalised to endogenous reference β-actin.
Determination of TNF-α and IL-6 levels
Mid-colon segments were homogenised in ice-cold physiological saline. The homogenates were centrifuged at 3000 g for 10 min and the supernatants were assayed for the determination of levels of the cytokines. The levels of each cytokine were evaluated using ELISA kits according to the manufacturer's protocols (R&D Systems), and the results are expressed in pg/mg of protein in each sample.
NF-κB nuclear translocation immunofluorescence
RAW264.7 cells were seeded in eight chamber slides (BD Biosciences) at a density of 5 × 104 cells per well. Cells were allowed to adhere at 37°C overnight and naringenin (25 μmol/l) was added for 2 h. Then, cells were overnight stimulated with lipopolysaccharide (2 μg/ml; Sigma-Aldrich) and fixed with 4 % (w/v) paraformaldehyde solution at 20°C for 10 min. After washing in PBS, cells were permeabilised with 0·3 % (w/v) Triton X-100 in PBS at room temperature for 20 min. After incubation in blocking buffer containing 0·1 % (w/v) Triton X-100, 1 % (w/v) bovine serum albumin and 3 % (w/v) donkey serum, cells were then incubated with rabbit NF-κB p65 antibody (#8242, 1:50; Cell Signaling) overnight at 4°C. After washing in PBS, cells were further incubated with Alexa Fluor 488-conjugated donkey anti-rabbit IgG (A-21 206, 1:500; Invitrogen) at room temperature for 45 min. In order to stain the nuclei, we added 1 μg/ml of 4′,6-diamidino-2-phenylindole (DAPI; Invitrogen) in PBS at room temperature. Fluorescence photographs were obtained using an Olympus CKX41 fluorescence microscope (Olympus Company).
NF-κB luciferase reporter assay
HT-29 cells were seeded in a twenty-four-well plate at a density of 1·5 × 105 cells/well at 1 d before transfection. The cells were transfected with 0·8 μg of pGL4.32 (luc2P/NF-κB-RE/Hygro) vector (Promega) using lipofectamine 2000 reagent (Invitrogen). The pGL4.32 plasmid is a NF-κB reporter vector. It contains NF-κB response elements and the firefly luciferase gene. At 12 h after the transient transfection, the cells were incubated with or without naringenin (1, 10 and 25 μmol/l) for 2 h, then treated with TNF-α (20 ng/ml; Cell Signaling) for an additional 5 h. At the termination of the experiments, cells were washed once with PBS, then lysed in 0·1 ml 1 × passive lysis buffer (Promega). Cell-free lysates were obtained by centrifugation at 10 000 g for 2 min at 4°C. The effects of naringenin and TNF-α on the activation of NF-κB promoter in transfected cells were determined by luciferase activity. Luciferase activity in cell lysate was quantified using a luciferase assay system (Promega) and a Glomax 20/20 luminometer (Promega). The results were presented as relative light units and data were expressed as fold values of control cells. Measurements were performed by calculating the average of quadruplicate samples of two independent experiments.
Statistical analysis
Data are expressed as the means and standard deviations. Statistical significance was analysed using a one-way ANOVA analysis followed by an independent t test. Statistical significance was considered when the P value was less than 0·05.
Results
Naringenin pre-administration attenuated dextran sulphate sodium-induced experimental colitis
There was no weight loss observed in mice receiving vehicle or naringenin alone (groups 1 and 2, respectively). The body weight of mice in group 3 dramatically decreased from day 3 onwards following DSS treatment. The mice receiving both DSS and naringenin (group 4) exhibited less significant weight loss than did the group 3 mice (Fig. 1(a)). Diarrhoea symptoms appeared on or shortly after day 3. At days 3–7, all the mice on the DSS-only treatment (group 3) experienced both diarrhoea and bloody diarrhoea, whereas none of the mice receiving vehicle or naringenin alone (groups 1 and 2, respectively) exhibited diarrhoea at any point during the study. By day 10, all the group 3 mice were euthanised due to critical weight loss. In contrast, the mice receiving both DSS and naringenin (group 4) exhibited less diarrhoea and bloody diarrhoea than did the group 3 mice (Fig. 1(b)). Colon shortening is an indirect marker of colonic inflammation(Reference Okayasu, Hatakeyama and Yamada21). After 7 d of treatment with DSS in drinking-water, there was a significant shortening (P= 0·038) of the colon length of mice in group 3 (5·5 (sd 0·4) cm, n 22) compared with the mice receiving both DSS and naringenin (group 4, 6·2 (sd 0·3) cm, n 28). This indicates that the oral administration of naringenin significantly ameliorated the symptom of colon shortening (Fig. 1(c)). Examination and scoring of colonic tissue samples from each group established that naringenin protected mouse mucosal epithelium from DSS-induced damage. Mice treated with vehicle or naringenin alone exhibited intact crypt–villus structures and epithelial layer. DSS administration resulted in a paucity of intact crypt–villus structures and large inflammatory exudates across the thickness of the bowel wall. By contrast, naringenin administration to DSS-exposed mice resulted in significant protection of the colon crypt structures and less severe histological inflammation (Fig. 1(d) and (e)).
Protective role of naringenin against dextran sulphate sodium (DSS)-induced colitis in mice. (a) Body weight changes following DSS induction of colitis. Data plotted as percentage of basal body weight. (b) The occurrence of bloody diarrhoea. Mice were evaluated for the occurrence of bloody diarrhoea following DSS administration. Data plotted as percentage of total mice that had bloody diarrhoea on different days (point of time) of DSS treatment. (c) Colon length. (d) Histological sections of mice exposed to DSS and/or naringenin showed healthy colon crypt structure for both vehicle treatment and naringenin treatment, but highly disrupted tissues in the DSS-only treatment group. In contrast, naringenin provided in combination with DSS protected the colon from DSS-induced damage. Original magnification 100 × . (e) Histological score of the distal colon. The distal colon is shown for the analyses of haematoxylin–eosin staining and pathohistological examination and scoring. Values are means and standard deviations of n 20 vehicle-treated mice, n 20 naringenin-treated mice, n 28 DSS-treated mice and n 29 naringenin+DSS-treated mice represented by vertical bars. Mean values were significantly different compared with DSS-treated group: * P< 0·05, ** P< 0·01, *** P< 0·001. ††† Mean values were significantly different compared with normal vehicle-treated group (P< 0·001). 
, Vehicle; 
, naringenin; 
, DSS+vehicle; 
, DSS+naringenin.
Naringenin inhibited Toll-like receptor 4 mRNA and protein expression
Growing evidence suggests that the TLR4/NF-κB signalling pathway plays a critical role in the pathogenesis of IBD. Therefore, targeted inhibition of the TLR4 signalling pathway in recent years has become a therapeutic strategy for IBD(Reference Liu, Li and Niu22, Reference Teng, Xu and Zhou23). To determine the effect of naringenin on TLR4 repression, quantitative real-time PCR and Western blot analyses were carried out. The results demonstrated that mRNA (Fig. 2(a)) and protein (Fig. 2(b) and (c)) expression of TLR4 were significantly induced in the colon mucosa after 7 d DSS treatment compared with the normal vehicle-treated group. The relative increase in mRNA and protein expression of TLR4 after DSS treatment was significantly less in mice pre-treated with naringenin (P< 0·01). The data indicate that naringenin might provide protection from DSS-induced colitis through suppression of TLR4 signalling.
Effect of naringenin on the expression of Toll-like receptor 4 (TLR4) mRNA and protein in the colon of dextran sulphate sodium (DSS)-induced colitis mice. (a) The mRNA expression of TLR4 was assessed by quantitative real-time PCR in mid-colon samples isolated from mice (n 6 per group) treated with vehicle, naringenin, DSS or naringenin+DSS. Experimental conditions were as described in the Materials and methods. Expression was normalised to β-actin, and each bar represents the means and standard deviations of triplicates of two independent experiments. (b) Mice (n 6 per group) were killed after 7 d of 4 % (w/v) DSS exposure, and total protein (40 μg) from mid-colon samples was loaded. Western blot was performed with anti-TLR4 (sc-293072, 1:1000) antibody. A representative experiment from three independent experiments is shown. (c) Quantification of the TLR4 protein expression was performed by densitometric analysis of the blot. Values are means and standard deviations of three independent experiments represented by vertical bars. Mean values were significantly different compared with DSS-treated group: ** P< 0·01, *** P< 0·001. Mean values were significantly different compared with vehicle-treated group: † P< 0·05, ††† P< 0·001.
Naringenin treatment blocked NF-κB activation in vivo and in vitro
NF-κB is viewed as a master switch in the regulation of inflammation and immunity. As a transcription factor, NF-κB controls an array of pro-inflammatory genes involved in the inflammatory signalling cascade(Reference Zhang, Cheng and Huang24, Reference Baeuerle and Henkel25). Based on this rationale, we hypothesised that the anti-inflammatory effect of naringenin in response to DSS-induced colitis correlated with blockade of NF-κB activation. A significant increase (P< 0·01) in the protein expression of phospho-p65 was observed in colonic tissues of the DSS-induced model group (Fig. 3(a) and (b)). Furthermore, the degradation and phosphorylation of IκBα was induced (P< 0·001) in colonic tissues of DSS-exposed mice compared with controls (Fig. 3(a) and (b)). By contrast, administration of naringenin reduced phospho-p65 expression in DSS-induced colitis, and the phosphorylation/degradation of IκBα was effectively suppressed (P< 0·01). In accordance with the in vivo data presented in Fig. 3(a) and (b), naringenin inhibited NF-κB p65 nuclear translocation, as indicated in lipopolysaccharide (2 μg/ml)-induced mouse macrophage RAW264.7 cells (Fig. 3(c)). On the other hand, induction of NF-κB-mediated luciferase activity in human colonic HT-29 cells by the inflammatory mediator, TNF-α (20 ng/ml), was inhibited by naringenin in a dose-dependent manner, reaching 80 (sd 13) % inhibition at 25 μmol/l (P< 0·001) relative to control cells (Fig. 3(d)). These results indicate that naringenin significantly blocked the NF-κB signalling pathway in experimental colitis by suppressing IκBα phosphorylation/degradation, blocking NF-κB p65 nuclear translocation and inhibiting NF-κB-mediated transcriptional activity.
Effect of naringenin on the suppression of NF-κB activity in vivo and in vitro. (a) Mice (n 6 per group) were killed after 7 d of 4 % dextran sulphate sodium (DSS) exposure, and total protein (40 μg) from mid-colon samples was loaded. Western blot was performed with anti-phospho-p65 (p-p65 (□); #3033, 1:1000) and anti-phospho-IκBα (p-IκBα (
); #2859, 1:1000) antibodies. One representative experiment from three independent experiments is shown. (b) Quantification of the p-p65 and p-IκBα protein expression was performed by densitometric analysis of the blot. Values are means and standard deviations of three independent experiments represented by vertical bars. (c) RAW264.7 cells were pre-treated with or without naringenin (25 μmol/l) for 2 h prior to lipopolysaccharide (LPS) (2 μg/ml) treatment for an additional 12 h. NF-κB p65 localisation was observed under a fluorescence microscope (magnification 200 × ) using an anti-NF-κB p65 antibody (#8242, 1:50) followed by an Alexa 488-conjugated detection antibody (A-21 206, 1:500). n 3. (d) HT-29 cells were transfected with pGL4.32 (luc2P/NF-κB-RE/Hygro) and then treated with TNF-α (20 ng/ml) for 5 h. For pre-treatment, cells were treated with naringenin (1, 10 or 25 μmol/l) for 2 h prior to TNF-α exposure. Cells were lysed and the lysate was analysed using a luciferase assay system. NF-κB promoter-driven luciferase activity was expressed as fold values of control cells (designated as 1). Values are means and standard deviations of quadruplicates of two independent experiments represented by vertical bars. Mean values were significantly different compared with the DSS-treated or TNF-α-treated group: ** P< 0·01, *** P< 0·001. Mean values were significantly different compared with the vehicle-treated group: † P< 0·05, †† P< 0·01, ††† P< 0·001.
Naringenin inhibited mRNA expression of pro-inflammatory mediators
To further determine the impact of naringenin on NF-κB signalling, we investigated the expression levels of representative downstream signalling genes involved in NF-κB activation. Quantitative real-time PCR analyses of several NF-κB target pro-inflammatory mediator genes were carried out. The results showed that mRNA expression of iNOS, ICAM-1, MCP-1, Cox2, TNF-α and IL-6 was remarkably induced (P< 0·001) in inflamed colons of mice exposed to DSS (group 3). In contrast, the increase in inflammatory regulators and mediators (iNOS, ICAM-1, MCP-1, Cox2, TNF-α and IL-6) following DSS treatment was significantly decreased (P< 0·01) in mice receiving naringenin administration (Fig. 4(a)–(f)). The results indicate that naringenin ameliorated DSS-induced colitis, which correlated with suppression of NF-κB signalling.
Effect of naringenin on the mRNA expression of pro-inflammatory mediator genes in the colon of dextran sulphate sodium (DSS)-induced colitis mice. The mRNA expression of (a) inducible NO synthase (iNOS), (b) intercellular adhesion molecule-1 (ICAM-1), (c) monocyte chemoattractant protein-1 (MCP-1), (d) cyclo-oxygenase-2 (Cox2), (e) TNF-α and (f) IL-6 was assessed by quantitative real-time PCR in mid-colon samples isolated from mice (n 6 per group) treated with vehicle, naringenin, DSS or naringenin+DSS. Experimental conditions were as described in the Materials and methods. Expression was normalised to β-actin, and values are means and standard deviations of triplicates of two independent experiments represented by vertical bars. Mean values were significantly different compared with the DSS-treated group: ** P< 0·01, *** P< 0·001. Mean values were significantly different compared with the vehicle-treated group: †† P< 0·01, ††† P< 0·001.
Naringenin reduced the production of TNF-α and IL-6 in colon
A significant increase (P< 0·001) in the content of TNF-α and IL-6 was observed in mice exposed to DSS (group 3) when compared with control mice (groups 1 and 2). Treatment with naringenin resulted in a reduction (P< 0·01) in the levels of TNF-α and IL-6 in mice receiving both DSS and naringenin (group 4) compared with DSS treatment model group (group 3) (Table 1). The data indicate that amelioration of inflammation in DSS-treated mice by naringenin treatment correlated with repression of pro-inflammatory cytokines.
The effect of naringenin on the production of colonic TNF-α and IL-6 in dextran sulphate sodium (DSS)-induced colitis mice‡ (Mean values and standard deviations of triplicates of two independent experiments)
Mean values were significantly different compared with the DSS-treated group: ** P< 0·01, *** P< 0·001.
† Mean values were significantly different compared with the vehicle-treated group (P< 0·001).
‡ Segments of mid-colon samples from mice (n 6 per group) were excised and homogenised. The supernatants were assayed for the determination of the levels of TNF-α and IL-6 using the ELISA method (R&D Systems).
Discussion
IBD consists of two distinct entities, Crohn's disease and ulcerative disease (UC). The main difference between Crohn's disease and UC is the location and nature of the inflammatory changes. Crohn's disease can affect any part of the gastrointestinal tract, from mouth to anus (skip lesions), although a majority of the cases start in the terminal ileum. UC, in contrast, is restricted to the colon and the rectum (continuous lesions). Microscopically, UC is restricted to the mucosa (epithelial lining of the gut), while Crohn's disease affects the whole bowel wall (transmural lesions)(Reference Huang, Chandra and Shih26, Reference van der Marel, Majowicz and van Deventer27). DSS, a heparin-like polysaccharide, has been widely used to induce both acute and chronic colitis in mouse models, with typical characteristics resembling human UC(Reference Shah, Ma and Morimura28, Reference Masubuchi and Horie29). The present study used an acute model of IBD by administration of DSS in drinking-water. The inflammation was mainly localised to the colon with features resembling human UC, such as ulceration, epithelial damage, mucosal inflammatory cellular infiltration and lymphoid hyperplasia(Reference Siddique and Khan30, Reference Singh, Chaturvedi and Barry31). The present results demonstrated that naringenin significantly abrogated colitis in a DSS-induced murine colitis model, and the beneficial effect of naringenin treatment could be linked, at least in part, to the inhibition of TLR4 protein and NF-κB activity, the down-regulation of expression of inflammatory mediators (iNOS, ICAM-1, MCP-1 Cox2, TNF-α and IL-6) and the inhibition of production of inflammatory cytokines (TNF-α and IL-6).
It is well-documented that NF-κB plays a pivotal role in the pathogenesis of IBD. Excess or inappropriate activation of NF-κB has been observed in human IBD(Reference Siddique and Khan30, Reference Andresen, Jørgensen and Perner32, Reference Schreiber, Nikolaus and Hampe33) and in the murine colitis model(Reference Shah, Ma and Morimura28, Reference Singh, Chaturvedi and Barry31). Inhibition of NF-κB activation with a specific p65 antisense oligonucleotide is an effective strategy in preventing experimental models of IBD(Reference Lawrance, Wu and Leite34) and in blocking inflammatory cytokine production in IBD patients(Reference Hibi, Inoue and Ogata35, Reference Li, Zhang de and Yi36). The NF-κB protein family consists of five members that include p50 and p65. These proteins form homo- and hetero-dimers, of which the p50/p65 heterodimer is the predominant NF-κB complex in most cells. In the absence of an inflammation-inducing stimulus, p50/p65 remains in an inactive state in the cytoplasm, forming a ternary complex with the inhibitory protein IκBα. Upon stimulation, IκBα is rapidly phosphorylated by IκB kinase, ubiquitinated and targeted for proteosome-mediated degradation. These events, thus, allow for the translocation of NF-κB p50/p65 to the nucleus, where it may bind with specific sequences located in the promoter of target genes and activate gene transcription(Reference Siddique and Khan30). NF-κB signalling is now considered a pivotal mechanism for the regulation of immune and inflammatory responses by controlling the transcription of inflammatory cytokine genes(Reference Siddique and Khan30). Thereby, NF-κB activation is believed to be an important step in the development of human IBD(Reference Schottelius and Baldwin37). Inhibition of NF-κB activation is associated with reduced colonic inflammation(Reference Atreya, Atreya and Neurath38). Many of the drugs used to treat human IBD (e.g. Sulfasalazine, infliximab and anti-TNF-α) inhibit NF-κB activation(Reference Zhao, Song and Hongzhu39, Reference Arijs, Li and Toedter40). It has also been reported that naringenin protects mice from asthma by preventing NF-κB activation(Reference Shi, Dai and Liu41). The present study confirms that naringenin protects mice from colitis by inhibiting NF-κB activation. Consistent with the in vivo data, our in vitro evaluation of NF-κB activity suggested a direct role of naringenin on blockade of lipopolysaccharide-stimulated NF-κB p65 nuclear translocation and TNF-α-induced NF-κB promoter luciferase expression. Due to a central role of NF-κB in inflammation, the blockade of NF-κB activation is thought to correspond to the breakage of the inflammatory signalling cascade(Reference Cheng, Shah and Ma42). Indeed, we found that administration of naringenin not only inhibited NF-κB activity, but also reduced the production of inflammatory cytokines (TNF-α and IL-6), down-regulated inflammatory mediators (iNOS, Cox2, ICAM-1 and MCP-1) and limited the inflammatory (histological) response. Together, these molecular changes result in significant amelioration of DSS-induced colitis.
Among many upstream signalling proteins involved in NF-κB activation, TLR4 plays a critical role(Reference Andersen, Christensen and Ernst43). As an innate immune receptor, TLR4 activates NF-κB through recruitment of the adaptor proteins MyD88 and TRIF, which leads to subsequent induction of NF-κB signalling genes, such as iNOS, Cox2, matrix metalloproteinase 9 (MMP-9), ICAM-1, MCP-1, TNF-α, IL-1, IL-6, IL-8, IL-15 and IL-27 (Reference Siddique and Khan30, Reference Joh and Kim44). Furthermore, TLR4 is up-regulated and NF-κB is activated during DSS-induced colitis in mice(Reference Fiorotto, Scirpo and Trauner15, Reference Liu, Li and Niu22, Reference Siddique and Khan30). Recent studies indicated that Lactobacillus suntoryeus, a gut commensal, blocks inflammatory mediators (Cox2, TNF-α, IL-1 and IL-6) through suppression of TLR4-linked NF-κB activation in mice with 2,4,6-trinitrobenzene sulfonic acid-induced colitis(Reference Lee, Lee and Lee45). In the present study, TLR4 was up-regulated in the colonic mucosa from mice with DSS-induced colitis; however, the up-regulation of TLR4 was significantly inhibited by naringenin administration. Indeed, there are preclinical strategies targeting TLR4 activity directly, which also result in significant abrogation of intestinal inflammation(Reference Ungaro, Fukata and Hsu11, Reference Fort, Mozaffarian and Stöver46). Thus, in light of the available literature on TLR4 and IBD, the present results support the hypothesis that naringenin appears to exert its effect in ameliorating DSS-induced colitis through blockade of the TLR4-linked NF-κB signalling pathway.
Other pathways, distinct from TLR4 and NF-κB, are also involved in the pathogenesis of IBD. For instance, recently we demonstrated that baicalein, a natural flavonoid and intestine-specific activator of human and mouse pregnane X receptor, abrogated DSS-induced colitis through a cdx2-mediated pregnane X receptor activation pathway(Reference Dou, Mukherjee and Li18). Shi et al. (Reference Shi, Dai and Liu41) showed that naringenin attenuated allergen-induced murine airway inflammation through NF-κB inhibition. Hämäläinen et al. (Reference Hämäläinen, Nieminen and Vuorela47) suggested that naringenin exposure blocked lipopolysaccharide-induced nuclear translocation of NF-κB in the mouse macrophage RAW264 and reduced iNOS expression. However, until recently, there has been no published evidence associating an interaction of TLR4 and naringenin or the rationale of the NF-κB pathway underlying the anti-colitis effect of naringenin. To our knowledge, for the first time, the present study demonstrates that TLR4-linked NF-κB signalling inhibition is an important mechanism underlying naringenin's anti-colitic effect in vivo. These results may give insight into the further evaluation of naringenin as a food supplement in the treatment of human IBD.
Acknowledgements
The present study was supported by the National Natural Science Foundation of China (81150040, U1032604), the Natural Science Foundation of Shanghai (12ZR1431400), the National Institutes of Health Grant RO1CA127231 (S. M.), the Damon Runyon Foundation Clinical Investigator Award (CI 1502) (S. M.) and the Albert Einstein College of Medicine. Author contributions are as follows: W. D. participated in study concept and design, acquisition of data, and analysis and interpretation of data; J. Z. aided in analysis and interpretation of data, acquisition of data, statistical analysis; and technical support; A. S. and E. Z. provided technical support, and aided in acquisition of data; L. D. participated in analysis and interpretation of data, and provided technical support; S. M. aided in study concept and design and critical review of the manuscript; X. W. aided in critical review of the manuscript for important intellectual content; G. C. provided material support and aided in critical review of the manuscript; Z.-T. W. provided material support, technical support, and aided in study supervision, administrative and obtained funding; S. M. aided in study concept and design, analysis and interpretation of compiled data, drafting of the manuscript and critical revision of the manuscript for important intellectual content. The authors have no conflicts of interest to declare.
