Casticin attenuates liver fibrosis and hepatic stellate cell activation by blocking TGF-β/Smad signaling pathway
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Ling Zhou1,*, Xiaoying Dong1,*, Linlin Wang1, Lanlan Shan2, Ting Li3, Wanfu Xu4, Yan Ding2, Mingqiang Lai5, Xiaojun Lin5, Meng Dai2, Xiaochun Bai5, Chunhong Jia5 and Hang Zheng1
1Department of Oncology, Nanfang Hospital, Southern Medical University, Guangzhou, Guangdong, China
2Department of Health Management, Nanfang Hospital, Southern Medical University, Guangzhou, Guangdong, China
3Department of Hepatobiliary Surgery, Zhujiang Hospital, Southern Medical University, Guangzhou, Guangdong, China
4Department of Gastroenterology, Guangzhou Women and Children’s Medical Center, Guangzhou Medical University, Guangzhou, Guangdong, China
5Department of Cell Biology, School of Basic Medical Sciences, Southern Medical University, Guangzhou, Guangdong, China
*These authors contributed equally to this work
Chunhong Jia, email: email@example.com
Hang Zheng, email: firstname.lastname@example.org
Keywords: casticin, CCl4, liver fibrosis, hepatic stellate cell, TGF-β/Smad
Received: May 24, 2016 Accepted: April 14, 2017 Published: April 27, 2017
Although many advances have been made in understanding the pathogenesis of liver fibrosis, few options are available for treatment. Casticin, one of the major flavonoids in Fructus Viticis extracts, has shown hepatoprotective potential, but its effects on liver fibrosis are not clear. In this study, we investigated the antifibrotic activity of casticin and its underlying mechanism in vivo and in vitro. Male mice were injected intraperitoneally with carbon tetrachloride (CCl4) or underwent bile duct ligation (BDL) to induce liver fibrosis, followed by treatment with casticin or vehicle. In addition, transforming growth factor-β1(TGF-β1)-activated LX-2 cells were used. In vivo experiments showed that treatment with casticin alone had no toxic effect while significantly attenuating CCl4-or BDL-induced liver fibrosis, as indicated by reductions in the density of fibrosis, hydroxyproline content, expression of α-SMA and collagen α1(I) mRNA. Moreover, casticin inhibited LX2 proliferation, induced apoptosis in a time- and dose-dependent manner in vitro. The underlying molecular mechanisms for the effect of casticin involved inhibition of hepatic stellate cell (HSC) activation and reduced the expression of matrix metalloproteinase (MMP)-2, MMP-9, tissue inhibitor of metalloproteinases (TIMP)-1 and TIMP-2 resulting from blocking TGF-β1/Smad signaling, as well as increased the apoptosis of HSCs. The results suggest that casticin has potential benefits in the attenuation and treatment of liver fibrosis.
Liver fibrosis is characterized by the excessive deposition of extracellular matrix (ECM) components, mainly fibrillar collagen, which occurs in most types of chronic liver diseases . This pathological status is the result of a dynamic process usually preceded by liver injuries such as chronic inflammation, viral hepatitis, alcohol abuse, metabolic liver diseases and others . If the injuries persist, fibrillar collagen accumulates, resulting in fibrosis and ultimately impairment of liver function. Advanced liver fibrosis results in cirrhosis, hepatocellular carcinoma, liver failure and portal hypertension[3, 4]. Although great progress has been made in elucidating the mechanisms underlying liver fibrosis, few options are available for its treatment [5–9].
Activated hepatic stellate cells (HSCs) are the major contributor to the production of fibrillar collagen in the injured liver . In the normal liver, HSCs are quiescent, residing in the space of Disse, and function as the main storage site of vitamin A. Following chronic injury, HSCs undergo a dramatic phenotypical transformation into α-smooth muscle actin (α-SMA)-positive myofibroblast-like cells and increase their expression of fibrillar collagen and matrix metalloproteinases (MMPs) such as MMP2 and MMP9, as well as tissue inhibitors of metalloproteinases (TIMPs). Consequently, fibrillar collagen accumulates, especially collagen I and collagen III. Increasing evidence indicates that transforming growth factor beta 1 (TGF-β1) is a key mediator in this pathogenesis by activating its downstream Smad signaling pathway [11–13]. According to differences in structure and function, Smads are classified into three groups. Smad2/3 are named receptor-activated Smads (R-Smads), and Smad4 is categorized as a common Smad (Co-Smad). Smads6, 7, and 8 are inhibitory Smads (I-Smad). When TGF-β1 binds to its receptor, Smad2/3 is phosphorylated and binds with Smad4, followed by translocation into the nucleus where these complexes activate transcription of profibrotic genes . Therefore, inhibiting the accumulation of activated HSCs by modulating either their activation and/or proliferation, or by promoting their apoptosis through the TGF-β/Smad signaling pathway, is a potential target for therapy [5, 15].
Many natural compounds have been shown to have hepatoprotective effects [16–18]. Vitex rotundifolia L. is a traditional herbal medicine in oriental countries. Its ripe fruits are called Fructus Viticis and have been used as folk medicine for headaches, colds, migraine and eye pain. Casticin(3′, 5-dihydroxy-3, 4′, 6, 7-tetramethoxyflavone) is one of the major flavonoids in Fructus Viticis extracts . It has been shown to have several biological activities, but most studies have focused on its anti-tumor effects in different types of cancer [20–24]. More recently, an anti-inflammatory effect by casticin has been reported in vitro and in vivo . Casticin has been shown to ameliorate cigarette smoke-induced acute lung inflammation and reduce croton oil-induced ear dermatitis and edema in mice . However, its effect on liver fibrosis has not yet been examined.
Here, to elucidate the potential effect of casticin on liver fibrosis in vivo, casticin was administered to mice that had received carbon tetrachloride (CCl4) injections or undergone bile duct ligation (BDL) to induce liver fibrosis. As we hypothesized, casticin prevented the activation of HSCs and reduced liver fibrosis in these two models. In order to determine the probable mechanisms, we also investigated the effects of casticin on TGF-β1-mediated HSC activation in LX2 cells from an immortalized human HSC cell line. We confirmed that casticin attenuated liver fibrosis probably by inhibiting the HSCs activation through TGF-β/Smad signaling pathway and inducing the apoptosis of HSCs. Our results suggest the potential of casticin as a new therapeutic drug for the treatment of hepatic fibrosis.
Casticin prevents hepatic injury induced by CCl4 or BDL in vivo
The in vivo effect of casticin on progression of fibrosis was assessed in two experimental mice models induced by CCl4 or bile duct ligation (BDL). In the first model, mice were given repeated injections of CCl4 for 6 weeks, and subsequently casticin (20 mg/kg) was administered by gastric gavage everyday for 2 weeks after the final CCl4 treatment. In the second model, mice underwent either sham operation or BDL. After BDL for 4 days, mice were administered intragastrically with casticin at 20 mg/kg/day(casticin dissolved in 0.25% Tween-80) or 0.25% Tween-80 for 2 weeks. Liver specimens were obtained 24 h after the last administration of casticin, and morphological changes of liver injury and fibrosis were visualized in sections stained by H&E. As expected, thick fibrotic septa and pseudolobular formation were more extensive in mice exposed to CCl4 or undergone BDL compared to controls (Figure 1A–1B). Similarly, the grades of fibrosis in the CCl4 and BDL fibrotic models were severe than controls (Figure 1C). Moreover, serum ALT, AST, albumin and total bilirubin were elevated in the CCl4 and BDL groups compared to controls (Figure 1D–1G). In contrast, treatment with casticin led to attenuation of both histological and functional injury. Mice treated with casticin alone displayed normal histology and serological values similar to the control mice. It indicated that treatment with casticin alone for two weeks had no toxic effect on the liver. These observations clearly demonstrate that casticin exerted a hepatoprotective effect.
Figure 1: Hepatoprotective effect of casticin in CCl4-and BDL-induced hepatic injury. Mice were given repeated injections of CCl4 for 6 weeks, and then given oral administration of casticin for 2 weeks. Representative photomicrographs of liver histology from normal healthy mice, casticin alone, CCl4 + vehicle alone and CCl4 + casticin (A) are shown. Other mice underwent BDL or sham operation for 4 days, and then were given oral administration of casticin or vehicle for 2 weeks. Representative photomicrographs of liver histology from sham, sham + casticin, BDL + vehicle alone, and BDL + casticin are shown (B). Grading of hepatic fibrosis was evaluated on a scale of 1–4 as follows: 1, scattered; 2, mild; 3, moderate and 4, marked. The histological changes were assessed in 200× magnification fields of slides stained with H&E (C). Serum aminotransferases, albumin and total bilirubin levels are plotted(D–G). The values are expressed as means ± SEM of eight determinations per group. **p < 0.01, ***p < 0.001.
Casticin attenuates liver fibrosis induced by CCl4 or BDL in vivo
Subsequently, the effect of casticin on alleviation of hepatic fibrosis was observed in liver sections stained by sirius red (Figure 2A–2B). Morphometric analysis of sirius red staining demonstrated that compared with control mice, CCl4 or BDL treatment caused a remarkable collagen accumulation in the liver, shown in Figure 2C. In contrast, treatment with casticin markedly decreased hepatic collagen matrix accumulation. Furthermore, the administration of casticin facilitated a decrease in hepatic hydroxyproline contents (Figure 2D). Collectively, these findings indicate that casticin attenuated hepatic fibrosis induced by CCl4 or BDL in vivo.
Figure 2: Effect of casticin on alleviation of CCl4-and BDL-induced hepatic fibrosis. (A–B) Histology with sirius red staining of liver sections (original magnification 100× and 400×). (C) Relative densitometry of fibrosis in mice. The density of fibrosis was determined as intensity of sirius red staining divided by the area of the captured field. A total of 24 fields were captured from livers in each group of mice. (D) Liver hydroxyproline content was determined to estimate collagen content, expressed as μg hydroxyproline per g liver tissue (wet weight). The values are expressed as means ± SEM (n = 8). **p < 0.01, ***p < 0.001.
Hepatic stellate cells are a major cell type responsible for liver fibrosis following their activation into fibrogenic myofibroblast-like cells, and α-SMA is an excellent marker for detection . As shown in Figure 3A, western blot analyses for α-SMA and vimentin were performed. α-SMA and vimentin protein expression were higher in the CCl4 and BDL groups compared with control groups, while the casticin treatment can reduce the expression sharply. In addition, immunohistochemical staining for α-SMA showed that α-SMA-positive cells were rarely detected in the control groups, but were clearly evident in the CCl4 and BDL groups. In sharp contrast, however, α-SMA-positive cells were markedly decreased in liver sections of CCl4 and BDL- injured mice treated with casticin (Figure 3B–3C). In fact, the number of α-SMA-positive cells per field was nearly 2-fold lower in the CCl4 + casticin group compared to the CCl4 group and nearly 4-fold lower in the BDL+ casticin group compared to the BDL group (Figure 3D). Furthermore, hepatic expression levels of collagen α1(I) mRNA were significantly decreased following casticin treatment (Figure 3E). Collectively, these findings suggest that casticin likely attenuated hepatic fibrosis induced by CCl4 or BDL in vivo probably by inhibiting HSC proliferation and activation.
Figure 3: Effect of casticin on proliferation and activation of HSCs. (A) Following the treatment previously described, the mice were euthanatized and their liver tissue was lysed and subjected to western blot analysis to assess α-SMA and vimentin. (B–C) Immunohistochemical staining of α-SMA. (D) Numbers of α-SMA positive cells were counted in 10 random low-power fields. Average numbers of positive cells in the fields are plotted (n = 8, ***p < 0.001). (E) Hepatic mRNA levels for collagen α1(I) were measured by real-time RT-PCR. The relative amounts of mRNA were normalized against GAPDH in the same samples (n = 8, **p < 0.01).
Casticin inhibits proliferation and induces apoptosis in LX2 cells
The LX-2 human hepatic stellate cell line has been widely characterized and maintains key features of hepatic stellate cytokine signaling, retinoid metabolism and fibrogenesis, making it a very suitable model of human hepatic fibrosis. To explore the underlying mechanisms for our in vivo observations, we carried out in vitro studies using LX-2 cells. We first confirmed that casticin inhibited proliferation of LX2 cells in a concentration-dependent manner (Figure 4A). Subsequently, the influence of casticin on LX2 cell apoptosis was assessed by morphological changes, AV-PI staining and flow cytometric assay. In the presence of 20 μM casticin, adherent LX2 cells began shrinking after 3 h; the majority of cells were detached from the dishes in 12 h (Figure 4B). And the AV-PI staining and flow cytometric assay results indicated that casticin induced cell apoptosis in a dose-dependent fashion (Figure 4D–4F). It was well known that cleavage of PARP facilitated cellular disassembly and served as a marker of cells undergoing apoptosis [28, 29]. Further, western blot analyses for cleaved PARP were performed (Figure 4C). Cleaved PARP was barely detectable in untreated LX2 cells, while specific bands corresponding to full-length PARP were clearly detected. In contrast, cleaved PARP was obviously detected in LX2 cells treated with 10 μM casticin for 1.5–6 h. Similar results were obtained in LX2 cells treated with 20 μM and 40 μM casticin. These findings strongly suggest that casticin inhibited LX-2 cell proliferation while promoting apoptosis in a time- and dose-dependent manner. Next, we explored the effect of casticin on L02 cells by cell proliferation assay and apoptosis analysis. We found that small dose(0–20 μM) casticin had no toxic effect on L02 cells. However, 40 μM casticin would suppresses L02 cells proliferation and induces apoptosis (Supplementary Figure 1B–1E).
Figure 4: Effect of casticin on cell proliferation and apoptosis of LX2 cells. (A) Cell proliferation was determined by CCK-8 assay. LX2 cells plated in 96-well plates were treated with casticin (5 μM, 10 μM, 20 μM or 40 μM) in growth medium containing serum for 48 h. (B) LX2 cells were cultured for 24 h, then incubated with casticin (20 μM) for up to 12 h. Representative phase-contrast photomicrographs of LX2 cells after incubation with equivoluminal DMSO or 20 μM casticin for 12 h are shown (original magnification 100× and 400×). (C) LX2 cells were cultured for 24 h, then treated with casticin (10 μM, 20 μM or 40 μM) for 0.5 h, 1.5 h, 3 h or 6 h. Cell lysates were subjected to western blot analysis to assess the cleavage of PARP. (D–F) LX2 cells were cultured for 24 h, then incubated with casticin (20 μM) for up to 12 h. Then casticin-induced cell apoptosis as measured by Annexin V–FITC and PI staining.
Casticin inhibits HSC activation and collagen matrix expression by blocking TGF-β/Smad signaling in LX2 cells
Since casticin inhibited cell proliferation and apoptosis, we next examined whether casticin could suppress HSC activation. It has been demonstrated that TGF-β1 is a classic activator of HSCs and a key mediator during development of liver fibrosis. Serum-starved LX-2 cells were treated with casticin for 12 h followed by TGF-β1 stimulation for 1 h. As expected, TGF-β1 increased LX-2 activation in control cells, as indicated by enhanced α-SMA expression, but this activation was suppressed in the presence of casticin. Meanwhile, the expression of α-SMA protein was assessed by immunofluorescence, which showed that the α-SMA expression increase under the TGF-β1 treatment, but this increase was attenuated by treatment with casticin (Figure 5A).
Figure 5: Effects and probable mechanisms of casticin on HSC activation in vitro. (A) Immunofluorescent detection of LX2 cells. Immunostaining was performed to detect expression of α-SMA (red, 600×) with nuclear counterstaining by DAPI (blue). (B) The phosphorylation level of Smad2/3 was analyzed by western blot. LX2 cells were plated in 24-well plates, incubated in serum-free medium for 12 h, followed by treatment with casticin in various concentrations (10–40 μM) for different durations (6 h/12 h) in the presence or absence of TGF-β1 (10 ng/μl) for 1 h. Cell lysates were subjected to western blot analysis. (C–H) TGF-β, collagen α1(I), MMP-2, MMP-9, TIMP1 and TIMP-2 mRNAs were measured by real-time RT-PCR (n = 5). *p < 0.05 vs. control, #p < 0.05 vs. TGF-β alone.
Previous studies have shown that TGF-β1 promotes the remodeling and deposition of ECM by activating downstream target genes such as MMPs and TIMPs. The TGF-β1-mediated signaling pathway depends on the phosphorylation of Smad2/3, which has been reported as a potential target for antifibrotic therapy [12–14, 27]. To understand the molecular mechanisms responsible for the inhibition of HSC activation, the protein activity of Smad2/3 (intracellular mediators of TGF-β1 signal transduction) was assessed. Western blot analysis showed significant increases in the phosphorylation of Smad2/3 stimulated by TGF-β1, and casticin treatment decreased the enhancement of phosphorylation by TGF-β1 (Figure 5B). We then confirmed that casticin inhibited the fibrotic effects of TGF-β1 on ECM deposition in LX2 cells by evaluating the mRNA levels of TGF-β, collagen α1(I), MMP-2, MMP-9, TIMP-1 and TIMP-2. Real-time PCR revealed that TGF-β1 significantly increased TGF-β, collagen α1(I), MMP-2, MMP-9, TIMP-1 and TIMP-2, but casticin reversed these trends (Figure 5C–5H). These results demonstrate that casticin inhibited TGF-β1-induced HSC activation and ECM remodeling.
Casticin inhibits HSC activation and collagen matrix expression by blocking TGF-β/Smad signaling in vivo
Finally, we identified potential antifibrotic mechanisms of casticin in vivo. Given that casticin can efficiently inhibit TGF-β1-induced HSC activation, we investigated the mechanism by which casticin attenuates CCl4-or BDL-induced liver fibrosis in vivo. As shown in Figure 6A and 6B, compared with control mice, CCl4-or BDL-induced liver fibrosis was accompanied by a marked activation of p-Smad3 (S423/425) and upregulation of TGF-β1 mRNA expression (Figure 6E), while casticin administration significantly decreased the phosphorylation of Smad3 and the level of TGF-β1 mRNA.
Figure 6: Effects and probable mechanisms of casticin on HSC activation in vivo. (A–B) Following treatment as previously described, the mice were executed, and their liver tissue were lysed and subjected to Western blot analysis to assess p-Smad3(S423/425), TIMP-1 and TIMP-2. Casticin administration decreased the phosphorylation of Smad3 and the level of TIMP-1. However, the protein expression of TIMP-2 did not show any difference between groups. (C–D) Zymography of liver lysates showing MMP-2 and MMP-9 gelatinase activity (upper panel) with densitometric quantification (lower panel). (E) Hepatic mRNA levels for TGF-β1 were measured by real-time RT-PCR. (F–I). Hepatic mRNA levels for MMP-2, MMP-9, TIMP-1 and TIMP-2 were measured by real-time RT-PCR.
The inhibitory function of casticin on the pro-fibrotic effects of TGF-β1 on ECM accumulation was further examined. Previous studies have demonstrated the MMPs and their endogenous TIMP inhibitors played a key role in ECM remodeling. Thus we first detected the serum MMP-2 and pro MMP-9 by Elisa, and the data illustrated that serum MMP-2 and pro MMP-9 was increased in the mice induced by CCl4 or BDL, but they were evidently decreased following casticin treatment (Supplementary Figure 2A–2B). Then to monitor the functional MMP-activity, gelatinase zymography have been performed. Compared to the mice induced by CCl4 or BDL, casticin administration showed a prominently decreased gelatinase activity (Figure 6C–6D). Real-time PCR test indicated the same trend in the mRNA expression of MMP-2, MMP-9, TIMP-1 and TIMP-2 (Figure 6F–6I). These results confirmed that casticin ameliorated experimental hepatic fibrosis by inhibiting HSC activation and collagen matrix accumulation through TGF-β/Smad signaling.
Hepatic fibrosis is a general consequence of chronic liver disease, and is characterized by a multicellular response with the activation of HSCs as a critical component. Therefore, inhibition of the accumulation of activated HSCs by modulating either their activation and/or proliferation, or by promoting HSC apoptosis, is the main target in patients with hepatic fibrosis . Recently, much interest in herbal medicine has been focused on the hepatoprotective or antifibrotic effects of compounds such as phyllanthus, silymarin, glycyrrhizin and sho-saiko-to . In this study, we first demonstrate that casticin has an inhibitory effect on liver fibrosis in vitro and in vivo as evidenced by the alleviation of fibrosis-related injury accompanied by reductions in collagen deposition and the number of α-SMA-positive cells, as well as diminished expression of profibrogenic markers in mouse fibrotic liver induced by CCl4 or BDL.
Casticin is one of the main components derived from the dried fruits of Vitex rotundifolia L. and has been used in prescriptions of traditional medicine for the treatment of colds, headache, migraine, sore eyes and other ailments. In 2004, Kobayakaw and colleagues confirmed that casticin disrupted mitotic spindles and showed that it had antimitotic effects on the human epidermoid carcinoma KB cell line without influencing the growth of normal cells . They suggested that G2-M arrest by casticin may inhibit microtubule dynamics. On this basis, casticin has been shown to inhibit the proliferation of breast cancer, lung cancer, colon cancer, human myelogenous leukemia cells and hepatocellular carcinoma cells in vitro [20–24, 31–33]. These findings suggest a similar anti-apoptotic inhibitory effect of casticin on rapid-proliferating cell types. In 2009, Choudhary and colleagues first reported the anti-inflammatory activities of casticin in vitro, and suggested their potential as non-steroidal anti-inflammatory agents . Recently, several studies have demonstrated that the anti-inflammatory effect of casticin is due to inhibition of pro-inflammatory cytokines and inflammatory mediators including NO and PGE2, blocking in turn the activation of NF-κB, Akt, and MAPK signaling . However, almost no information is available regarding the anti-fibrotic effects of casticin on liver fibrosis. Our in vivo study using two mouse models of liver fibrosis induced by carbon tetrachloride and bile duct ligation indicated that casticin exerted hepatoprotective and anti-fibrotic effects. In vitro, we also showed that casticin could inhibit the proliferation and induce apoptosis in the LX2 human hepatic stellate cell line. Our results were consistent with the previous studies that showed the casticin have key roles in regulating cell proliferation and apoptosis.
The molecular mechanism of cell activation in HSCs has recently been extensively investigated [1–6]. In our study, we characterized inhibition of TGF-β1 signaling most likely plays an essential role in the anti-fibrotic effect of casticin. Since TGF-β1 is one of the key regulators of HSC activation , it is also possible that casticin inhibits autocrine/paracrine signaling in activated HSCs, thereby facilitating resolution of CCl4- or BDL-induced hepatic fibrosis in vivo. In addition, it has been postulated that the constitutive activation of TGF-β1 signaling is one of the main factors acting as a cell-survival signal in activated HSCs . Indeed, most chemicals which suppress the activation of HSCs have been shown to inhibit TGF-β1 signaling [35–36]. Our studies concluded the same results. Furthermore, our experiments also indicated the casticin had the pro-apoptotic effect on HSCs. It has been reported that casticin could induce apoptosis through NF-κB, ASK1-JNK-Bim and mitotic arrest in many types of tumour cells [19–24], however, it was unclear the apoptosis could be induced by TGF-β/Smad signaling pathway especially in the activated HSCs . Although our study indicated these results, we could not make sure to draw this conclusion. Further experiments need to be carried on.
In conclusion, casticin suppresses the activation of HSCs and induces apoptosis in activated HSCs both in vitro and in vivo. Although a complete understanding of the molecular mechanisms will require further investigation, it is likely that casticin inhibits TGF-β1 signaling pathways, leading to a reduction in downstream phosphorylation of Smad2/3 that inhibits HSC activation. Future approaches examining clinical applications of casticin are promising for the establishment of a new treatment for hepatic fibrosis in a variety of chronic liver diseases.
MATERIALS AND METHODS
Sirius red was obtained from Sigma-Aldrich (St. Louis, MO, USA). CCl4 was purchased from Aladdin Industrial Corporation (Shanghai, China). Casticin was purchased from Chengdu Biopurify Phytochemicals Ltd. (Chengdu, China). Casticin has a molecular weight of 374.3 kDa, appears as yellow crystals and had a purity of 98.0%. Antibodies against glyceraldehyde-3-phosphate dehydrogenase (GAPDH) and HRP-conjugated anti-mouse and anti-rabbit IgG were obtained from Sigma-Aldrich. Antibodies against vimentin, phospho-Smad2 (S465/467), phospho-Smad3 (S423/425) and poly (adenosine diphosphate-ribose) polymerase (PARP), TIMP-1 and TIMP-2 were purchased from Cell Signaling Technology (Danvers, MA, USA), and antibody against α-SMA was purchased from Abclonal Technology (Wuhan, China).
Animal models of liver fibrosis
CCl4 intraperitoneal injection
Male mice 6–8 weeks of age weighing 20–30 g were purchased from Southern Medical University Experimental Animal Center (Guangzhou, China) and kept in a temperature-controlled room with an alternating 12 h dark and light cycle. All procedures involving animals in this study were approved by the animal care committee of Southern Medical University in accordance with institutional guidelines for animal experiments. A total of 32 mice were divided randomly into four groups of 8 animals each: control, casticin, CCl4, and CCl4 + casticin. To induce liver fibrosis, CCl4 dissolved in olive oil (20%) was injected intraperitoneally into mice (1.0 ml/kg body weight) in the CCl4 and CCl4 + casticin groups twice a week for six weeks. Mice in the control group and casticin group were injected with an equivalent volume of olive oil. Casticin was dissolved in 0.25% Tween-80. After treatment with CCl4 or olive oil for six weeks, mice in the casticin group and CCl4 + casticin group received casticin (20 mg/kg) by gastric gavage daily for two weeks, and the other two groups were given the equivalent volume of 0.25% Tween-80. After the eight week intervention period, mice were euthanatized under 3% pentobarbital sodium anesthesia (40 mg/kg ip), and the livers and blood from all animals were collected. Serum was obtained by centrifugation (1600 g, 15 min) and stored at −20oC for further examination.
Bile duct ligation surgery
Male mice 6–8 weeks of age weighing 20–30 g underwent either sham operation or bile duct ligation (BDL) . A total of 32 mice were divided randomly into four groups of 8 animals each: control, casticin, BDL, and BDL + casticin. In sham operation, the bile duct was exposed, but not ligated. After BDL for 4 days, mice were administered intragastrically with casticin (n = 8) at 20 mg/kg/day or 0.25% Tween-80 (n = 8) for 2 weeks. Liver samples from these mice were collected within 24 h after the last administration of casticin. The samples were snap-frozen in liquid nitrogen and stored at −80°C until used.
Serum aminotransferases, albumin and total bilirubin
Serum levels of alanine aminotransferase (ALT), aspartate aminotransferase (AST), albumin and total bilirubin were determined by Catalyst Dx™ Chemistry Analyzer (Yeeran Technology Limited, Beijing, China).
Serum MMP-2 and pro MMP-9 determination
Mouse MMP-2 and pro MMP-9 Elisa Kit are the enzyme-linked immunosorbent assay for measuring mouse MMP-2 and pro MMP-9 in serum. Mouse MMP-2 Elisa Kit and Mouse pro MMP-9 Elisa Kit were purchased from Thermo Scientific (Frederick, USA).
Liver histology and morphometric collagen determination
The livers were fixed in 4% paraformaldehyde and embedded in paraffin, sectioned at 4 μm and stained with hematoxylin-eosin (H&E) and sirius red. The extent of fibrosis was evaluated on blinded slides by a member of our Department of Pathology. Fibrosis was determined histologically by measuring the intensity of fibrosis in five (magnification 100×) digital images captured from slides of each mouse stained with sirius red. The total fibrosis density score was determined by dividing the image intensity by the image area as described in reference .
Determination of hepatic hydroxyproline content
The hepatic hydroxyproline content as an indirect measure of tissue collagen content was expressed as μg/gram of liver wet weight. It was measured by using a hydroxyproline detection kit (Jiancheng Institute of Biotechnology, Nanjing, China) according to the manufacturer’s instructions.
MMP-2, 9 activity were assessed by gelatin zymography as described before [39–40]. For gelatin zymography 1 mg/mL gelatin was copolymerized in a 7.5% PAGE gel and 20 μg protein of pooled liver lysates of each group was loaded.
After deparaffinization and dehydration, microwave antigen retrieval was performed, followed by peroxidase quenching. Subsequently, the sections were blocked with goat serum for 1 h at room temperature and incubated overnight at 4°C with 1:100 dilutions of primary antibodies to α-SMA. Negative control sections were treated identically, except for omission of the primary antibodies. After washing in PBS, the sections were incubated with HRP-conjugated secondary antibodies for 1 h at room temperature, and immunoreactivity was visualized with 3,3′-Diaminobenzidine (DAB) staining. Finally, slides were counterstained with Harris hematoxylin. For quantitation of immunoreactivity, 15 consecutive nonoverlapping fields at 200× magnification were scored using a graticule eyepiece in a blinded fashion.
LX 2 cells, an immortalized human HSC cell line, were purchased from KeyGEN BioTECH (Jiangsu, China). Cells were cultured in RPMI-1640 medium supplemented with 10% fetal bovine serum and incubated at 37°C in a humidified air atmosphere containing 5% CO2. Morphological changes after indicated treatments were observed by regular phase contrast microscope.
To evaluate the effect of casticin on LX-2 cells using real-time PCR and western blot analysis, cells were serum-starved overnight, then treated with 10 ng/μl TGF-β1 for 30–60 min in the presence or absence of casticin for the indicated time periods (0.5–12 h). The casticin was dissolved with dimethylsulfoxide (DMSO) , then diluted to determined concentration with culture medium.
Cell proliferation assay
LX-2 cells or L02 cells were plated at a density of 5 × 103 cells per well in a 96-well plate and treated with casticin (0–40 μM) for 48 h in growth medium containing serum. Cell proliferation was determined using a CCK-8 assay kit (Dojindo, Tokyo, Japan) according to the manufacturer’s instructions.
To quantitatively assess the rate of apoptosis, AV-PI staining was conducted. We used Annexin V/propidium iodide double-labelled flow cytometry kit (KeyGen, Nanjing, China) as the manufacturer described. Briefly, 2 × 105 LX2 cells or L02 cells were treated with casticin (0–40 μM) for 12 h, respectively. After harvested and washed twice with PBS, the cells were resuspended in 500 μl binding buffer. Then, 5 μl of annexin V and 5 μl of PI were added. The mixture was incubated at room temperature for 5 min in the dark. Then cells were analysed by flow cytometry with a Becton Dickinson FACS-420 flow cytometer (Franklin Lakes, NJ, USA).
LX-2 cells were grown on chamber slides and treated with casticin and TGF-β1 as previously described. The cells were fixed in 4% paraformaldehyde/PBS (10 min) and then incubated in 1% BSA/10% normal goat serum in 0.1% PBS-Tween for 1 h to permeabilize the cells and block non-specific protein interactions. The cells were then incubated with antibody against α-SMA at 10 μg/ml overnight at 4°C. The secondary antibody (red) was Alexa FluorR 594-labeled goat anti-mouse IgG used at a 1/500 dilution for 1 h. Diamidino-phenyl-indole (DAPI) was used to stain the cell nuclei (blue) at a concentration of 1.43 μM. After washing with PBS four times for 15 min, cells were mounted and analyzed by fluorescence microscopy (magnification 200×).
Gene expression analysis by quantitative real-time PCR
Total RNA was isolated from liver tissue in mice and from LX-2 cells using Trizol reagent (Invitrogen, Carlsbad, CA, USA). RNA (1 μg) was reverse-transcribed using a reverse transcription-polymerase chain reaction (RT-PCR) kit (Promega, Madison WI, USA) to obtain cDNA. Real-time PCR was carried out using the 7500 real-time PCR system (Applied Biosystems, Foster City, CA, USA) using a SYBR Green PCR Kit (TaKaRa, Shiga Prefecture, Japan). The Cp value of α1(I) collagen, TGF-β1, MMP-2, MMP-9, TIMP-1 and TIMP-2 was normalized based on that of GAPDH using 7500 System SDS Software Version 1.2 (Applied Biosystems). A melting curve analysis was done after amplification to verify the accuracy of the amplicon. The primer pairs used were listed in Table 1.
Table1: Primer sequences and accession numbers for primers used for RT-PCR
Forward Primer (5′–3′)
Reverse Primer (5′–3′)
Western blot analysis
Cells were lysed in 2×SDS sample buffer (adding protease inhibitors and phosphatase inhibitor) on ice. Equal amounts of whole protein extract were resolved by SDS-PAGE, transferred to a nitrocellulose membrane and probed overnight at 4°C with primary antibodies. Membranes were washed with TBS/0.05% Tween-20 and incubated with HRP-conjugated secondary antibodies at room temperature for 1 h. Proteins were detected by enhanced chemiluminescence substrates (PerkinElmer, Massachusetts, USA).
All data were expressed as mean±SEM Student’s t test or two-way analysis of variance was used to analyze differences between groups. A value of P < 0.05 was considered statistically significant.
CCl4, carbon tetrachloride; α-SMA, α-smooth muscle actin; PARP, poly (adenosine diphosphate-ribose) polymerase; HSC, hepatic stellate cell; MMP, matrix metalloproteinase; TIMP, tissue inhibitor of metalloproteinases; TGF-β1, transforming growth factor beta1; ECM, extracellular matrix; ALT, alanine transaminase; AST, aspartate aminotransferase; DAB, 3,3'-Diaminobenzidine; DAPI, diamidino-phenyl-indole; RT-PCR, real time-polymerase chain reaction; Col1α1, collagen type1 alpha 1.
The work was supported by the National Natural Science Foundation of China (No. 81301525), Natural Science Foundation of Guangdong Province (No. 2014A030313297 and No. 2016A030313556).
CONFLICTS OF INTEREST
The authors do not have any disclosures to report.
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