Ham’s F-12K medium and fetal bovine serum were purchased from the American Type Culture Collection (ATCC, Manassas, VA, USA). STC was obtained from Sigma Chemical Co. (St. Louis, MO, USA). Emodin was purchased from Solarbio Science and Technology Co. (Beijing, China). Rhodamine 110, bis-(CBZ-L-isoleucyl-l-prolyl-l-arginine amide) dihydrochloride (BZiPAR), and the EnzChek^® Ultra Amylase Assay Kit were purchased from Molecular Probes^® Labeling and Detection Technologies (Waltham, MA, USA). Tumor necrosis factor alpha (TNF-α), interleukin-1 beta (IL-1β), and interleukin-6 (IL-6) enzyme-linked immunosorbent assay (ELISA) kits were obtained from Lengton Biotech (Shanghai, China). RNAiso Plus reagent, PrimeScript^® RT reagent and SYBR^® PremixEx Taq™ II (TliRNaseH Plus) were purchased from TaKaRa Biotechnology Co., Ltd. (Dalian, China). The lactate dehydrogenase (LDH) assay kit was obtained from the Nanjing Jiancheng Institute of Biotechnology (Nanjing, China). The protein extraction kit was purchased from KEYGEN Biotech. Co., Ltd. (Nanjing, China). The bicinchoninic acid (BCA) protein assay kit was purchased from the Beyotime Institute of Biotechnology (Shanghai, China). Hoechst 33342 was obtained from Solarbio (Beijing, China). The Double-Luciferase Reporter Assay Kit was obtained from TransGen Biotech (Beijing, China). HTRA1-WT/MUT plasmid, lipofectamine 2000, and miR-30a-5p mimic and inhibitor were obtained from RiboBio Co., Ltd. (Guangzhou, China). The HTRA1-pcDNA3.1 plasmid, TGF-β1-pGL3-Basic, and miR-30a-5p antagomir were purchased from GenePharma Corp. (Shanghai, China). Rabbit anti-HTRA1, TGF-β1, interleukin-33 (IL-33), myeloid differentiation primary response gene 88 (MyD88), TNF receptor-associated factor-6 (TRAF-6), and NF-κB, horseradish peroxidase-conjugated goat anti-rabbit IgG, and TRITC-conjugated goat anti-rabbit IgG (H + L) were purchased from the Proteintech Group (Chicago, IL, USA). Mouse anti-monoclonal myeloperoxidase (MPO) antibody (FITC) was obtained from Abcam (Cambridge, UK).

AR42J rat pancreatic acinar cells (ATCC^® CRL-1492™), purchased from ATCC, were maintained in Ham’s F-12K medium supplemented with 20% fetal bovine serum in a humidified atmosphere of 5% CO₂ at 37°C.

Cells were cultured in 96-well plates at a density of 1 × 10⁵ cells⋅mL⁻¹ for 48 h and were then challenged with various concentrations of STC (16,000, 8,000, 4,000, 2,000, 1,000, 500, 250, 125, and 62.5 µM) for 1 h. Cell viability was assessed to determine the most suitable concentration of STC using the MTT method (26). Briefly, the plates were incubated with MTT solution (5 mg⋅mL⁻¹) for 4 h at 37°C, and subsequently, 100 µL of dimethyl sulfoxide was added to dissolve the formazan crystals. Finally, the absorbance was measured at 490 nm using a microplate reader (Thermo, Waltham, MA, USA); and the data were performed log transformation in order to generate half maximal inhibitory concentration (IC50) curve for parametric analysis.

AR42J cells were cultured in 96-well plates at a density of 1 × 10⁵ cells·mL⁻¹ for 48 h and were then treated with various concentrations of emodin (80, 60, 40, and 20 µM) for 2 h at 37°C. Subsequently, the cytotoxicity of this compound was assayed through the detection of released LDH at 450 nm using a microplate reader (Thermo, Waltham, MA, USA) according to the manufacturer’s instructions.

AR42J cells were cultured in 96-well plates at a density of 1 × 10⁵ cells·mL⁻¹ for 48 h and then pretreated with various concentrations of emodin (40, 20, 10, 5, 2.5, 1.25, and 0.625 µM) for 2 h before being challenged with STC (498.2 µM) for 1 h. The cells in the model group were cultured without emodin, and the cells in the control group were cultured under normal conditions. The MTT method was used to assay cell viability as described above. Furthermore, AR42J cells were grown in six-well plates and treated with various concentrations of emodin (10, 20, and 40 µM) for 2 h at 37°C before being challenged with STC (498.2 µM) for 1 h; cell morphology was then imaged using a phase contrast microscope (Nikon, Chiyoda pill, Tokyo, Japan).

In preparation for intracellular proteinase assays with rhodamine 110-based substrates, AR42J cells were incubated with HEPES-buffered saline (HBS; 5 mM HEPES and 0.15 M NaCl, pH 7.35) containing 2 mM EDTA (HBS-EDTA) and stored at 4°C for no longer than 2 h after removing the different media. Subsequently, the cells were incubated for approximately 20 min in the presence of 10 µM substrates. Finally, trypsin activity was investigated using laser confocal microscopy with 400× magnification (Leica, Wetzlar, Germany).

An EnzChek amylase assay kit was used to determine the quantitative kinetic activity of α-amylase in the supernatant samples from all of the AR42J cell cultures. Fifty microliters of each sample were added into 200 µg·mL⁻¹ DQ starch substrate solution in a 96-well plate according to the EnzCheck protocol. The samples were incubated at room temperature, protected from light, for an appropriate amount of time (10–30 min). The relative fluorescence intensity was read at 505 nm using a multifunctional microplate reader (BioTek, Winooski, VT, USA).

AR42J cells were cultured in six-well plates for 48 h and then treated with different media. Immunofluorescence measurements of HTRA1 were performed as previously described (26). The cells were incubated with diluted HTRA1 antibody (1:100) overnight, followed by TRITC-conjugated goat anti-rat IgG (H + L) for 1 h at 37°C; subsequently, the cells were restained with Hoechst 33342 (1 µg·mL⁻¹) for 5 min. Digital images were collected using an Olympus BX63 fluorescence microscope (Olympus; Tokyo, Japan) at 200× magnification. The fluorescence intensity of the images was quantified using image-Pro Plus 6.0 software (Media Cybernetics, Inc., Rockville, MD, USA).

AR42J cells were seeded onto six-well plates (1 × 10⁵ cells·mL⁻¹) in a serum-free medium and transfected with HTRA1-pcDNA3.1 mixed with lipofectamine 2000 according to the manufacturer’s instructions. In addition, 24 h after transfection, the cells were cultured in the presence or absence of emodin (40 µM) for 2 h before being challenged with STC (498.2 µM) for an additional 1 h. Subsequently, the protein levels of HTRA1, TGF-β1, IL-33, MyD88, TRAF-6, and NF-κB; the mRNA levels of TNF-α, IL-1β, and IL-6; and the supernatant contents of amylase, lipase, TNF-α, IL-1β, and IL-6 were measured.

MicroRNAs are important regulators of gene expression. To elucidate the potential mechanism by which emodin protects against pancreatitis, candidate upstream miRNAs that target rat HTRA1 mRNA were identified in the miRanda, miRDB, TargetScan, and CLIP databases. The miRNAs from the four databases were further screened, and the resulting candidate miRNAs listed in Table S1 in Supplementary Material were predicted by several software programs. Furthermore, the TargetScan 7.1 database predicted that bases 366–373 in the 3′-UTR of HTRA1 constitute a possible binding site for miR-30a-5p.

For the dual luciferase reporter assay, the 3′-UTR of HTRA1 was cloned into the pmiR-RB-REPORT™ vector to construct the wild-type (WT) 3′-UTR. Site-directed mutagenesis of the miR-30a-5p binding site in the HTRA1 3′-UTR was performed to make a mutant (MUT) 3′-UTR. Plasmids containing the WT miR-30a-5p-HTRA1 response element (HTRA1-WT) and the corresponding mutant (HTRA1-MUT) were purchased from RiboBio Co., Ltd. (Guangzhou, China). AR42J cells were co-transfected with plasmid DNA (HTRA1-WT or HTRA1-MUT) and miR-30a-5p mimic (50 nM) or the negative control for 24 h. The sequences of the miR-30a-5p mimic are listed in Table S2 in Supplementary Material. Luciferase activities were then assessed using a Double-Luciferase Reporter Assay Kit with a multifunctional microplate reader (BioTek, Winooski, VT, USA), normalized to the ratio of Firefly and Renilla luciferase signals. Furthermore, 24 h after transfection with HTRA1-WT/MUT plasmids and miR-30a-5p mimic, respectively, the HTRA1 protein level in AR42J cells was detected by western blotting to confirm whether HTRA1 is the target protein of miR-30a-5p.

In addition, plasmids containing HTRA1 (HTRA1-pCDNA3.1) and the TGF-β1 promoter (TGF-β1-pGL3-Basic) were purchased from GenePharma Inc. (Shanghai, China). HTRA1-pCDNA3.1 or TGF-β1-pGL3-Basic and miR-30a-5p mimic/inhibitor were co-transfected into AR42J cells for 24 h. The sequences of the miR-30a-5p inhibitor are listed in Table S2 in Supplementary Material. The dual luciferase reporter assay was then conducted as described above.

Total miRNA from AR42J cells treated with or without emodin was extracted using an EasyPure^® miRNA Kit (TransGen Biotech, China) according to the manufacturer’s instructions. Reverse transcription was performed using the TransScript^® One-Step gDNA Removal and cDNA Synthesis SuperMix (TransGen Biotec, Beijing, China) according to the manufacturer’s instructions in a TC-512 PCR system (TECHNE, Cambridge, UK), and the levels of mature miRNA were quantified using real-time PCR with the TransScript^® Top Green qPCR SuperMix (TransGen Biotec, Beijing, China) in an ABI 7500 Real-Time PCR System (Applied Biosystems, Foster, CA, USA), and the U6 small nucleolar RNA was used for normalization. The pre-primers and post-primers (RN: R10031.4) of miR-30a-5p and U6 were obtained from RiboBio Co., Ltd. (Guangzhou, China).

AR42J cells were seeded onto 6-well plates (1 × 10⁵ cells·mL⁻¹) in a serum-free medium and transfected with miR-30a-5p inhibitor (100 nM) mixed with lipofectamine 2000 for 24 h according to the manufacturer’s instructions. miR-30a-5p inhibitor sequence is listed in Table S2 in Supplementary Material. After transfection, the cells were treated with different media, and subsequently, the protein levels of HTRA1, TGF-β1, IL-33, MyD88, TRAF-6, and NF-κB, the mRNA levels of TNF-α, IL-1β, and IL-6, and the supernatant contents of amylase, lipase, TNF-α, IL-1β, and IL-6 were measured.

All animal care and experimental procedures in the present study were approved by the Animal Care and Use Committee at Dalian Medical University and were performed in strict compliance with the People’s Republic of China Legislation Regarding the Use and Care of Laboratory Animals. Rats were obtained from the Experimental Animal Center at Dalian Medical University (Dalian, China) and maintained with a 12-h light–dark cycle in a temperature-controlled (25 ± 2°C) room. All the animal studies complied with the principle for replacement, refinement, or reduction (the 3Rs). The animals were housed in groups with three rats per cage with free access to standard laboratory food and water, and they were acclimatized for 1 week prior to the experiment.

Thirty male Sprague-Dawley (SD) rats weighing 180–220 g (6–8 weeks old) were randomly divided into five groups (n = 6, where “n” refers to the number of animals in each group): Group I, sham operation group (control); Group II, pancreatitis model group; Group III, emodin-treated group (60 mg·kg⁻¹); Group IV, antagomir group; and Group V, antagomir + emodin group. Using an antagomir, a synthetically derived oligonucleotide sequence that complementary binds to the miRNA, it was able to inhibit miR-30a-5p activity and alleviate rejection in rats. And, the miR-30a-5p antagomir sequence is listed in Table S2 in Supplementary Material. Rats in the antagomir and antagomir + emodin groups were injected with antagomir (20 µmol·kg⁻¹·day⁻¹) in the tail vein for 3 days, and experimental models were established 1 h after injection on the last day as previously described (27). Briefly, animals were fasted for 12 h with free access to water and then anesthetized. Pancreatitis was induced by standard retrograde infusion of freshly prepared 5.0% STC (0.1 mL per 100 g body weight) into the biliopancreatic duct. The control group received a retrograde infusion of an equivalent volume of sterile saline. After establishing the animal model, emodin was intragastrically administered to the rats in the emodin and antagomir + emodin groups immediately and again after 6 h. Both the control and model groups were administered an equivalent volume of 0.5% carboxymethylcellulose sodium (CMC-Na). Blood samples were collected via the abdominal aorta of the rats for biochemical analyses after 12 h of duct infusion and anesthesia. Pancreatic head samples were fixed in 10% buffered formalin and embedded in paraffin for histopathological examination and immunofluorescence examinations. The other pancreas samples were immediately frozen and maintained at −80°C for real-time PCR and western blotting analyses.

Formalin-fixed tissue samples from all of the groups were stained with hematoxylin and eosin (HE) and examined using light microscopy (Leica, Wetzlar, Germany) at 200× magnification. Typical images were collected, and the effects of emodin on pancreatic edema, inflammation, and vacuolization were evaluated. We applied a scoring system as shown in Table S3 in Supplementary Material.

Immunofluorescence localization of MPO and HTRA1 was performed with pancreas sections using previously described methods (27). After the slides were treated with mouse anti-MPO antibody (FITC) and rabbit anti-HTRA1 antibody overnight, they were then incubated with TRITC-conjugated goat anti-rabbit IgG (H + L) for 1 h at 37°C. Subsequently, the cells were restained with Hoechst 33342 (1 µg·mL⁻¹) for 5 min. Digital images were obtained using an Olympus BX63 fluorescence microscope (Olympus BX63, Japan) at 200× magnification.

The supernatant and plasma were collected from AR42J cells and rats after the experiments. Amylase, lipase, TNF-α, IL-1β, and IL-6 levels in the supernatant or plasma were assayed with ELISA kits according to the manufacturer’s instructions.

Total RNA from AR42J cells and rat pancreas samples was extracted using the RNAiso Plus reagent according to the manufacturer’s instructions. Quantitative real-time PCR assay was conducted as described above. The primer sequences are listed in Table S4 in Supplementary Material. All gene expression levels were normalized to GAPDH, and the fold changes between the different groups were calculated using a standard curve for quantitative analysis.

Total protein was extracted from AR42J cells and pancreas tissues using cold lysis buffer (containing 20 mM Tris, pH = 7.5, 150 mM NaCl, 1% Triton X-100, sodium pyrophosphate, β-glycerophosphate, EDTA, Na₃VO₄ and leupeptin) supplemented with 1 mM phenylmethyl sulfonyl fluoride, and their protein concentrations were determined using a BCA protein assay kit. The samples were separated using SDS-PAGE (10–15%) and transferred onto PVDF membranes (Millipore, USA). The membranes were blocked and incubated overnight at 4°C with primary antibodies for HTRA1, TGF-β1, IL-33, MyD88, TRAF-6, and NF-κB. The membranes were then incubated at room temperature with secondary antibodies, and protein expression was visualized using a ChemiDoc XRS Bioimaging System (Bio-Rad, USA). To eliminate variations in protein expression, the data were adjusted to the expression level of the corresponding internal reference [the integrated optical density (IOD) value of target protein versus the IOD of GAPDH].

The data were expressed as the mean ± SD from three or more independent experiments. Statistical analysis was performed with GraphPad Prism 6.0 software (Graphpad Software, Inc., San Diego, CA, USA). One-way ANOVA/Kruskal–Wallis tests followed by post hoc Tukey’s/Dunn’s (according to homogeneity of variances: yes/no) were used for the analysis of the differences between multiple independent groups, and the unpaired t-test/Mann–Whitney U test was carried out for two different groups’ comparison (according to homogeneity of variances: yes/no). Post hoc tests were performed when ANOVAs indicated that a significant difference existed between groups. p values of <0.05 or <0.01 were considered statistically significant.

In order to choose the proper stimulus concentration, the viability of AR42J cells treated by different STC doses was detected through MTT assay, and the results showed that the IC50 of STC after 1 h treatment was 498.2 µM (Figure 1A), which was selected as the stimulus dose for the in vitro model. In addition, the cytotoxicity of emodin against AR42J cells was detected using LDH testing, and the results showed that 60 µM emodin had obvious cytotoxicity (p < 0.05); therefore, a maximum dose of 40 µM emodin was used in the following experiments (Figure 1B). As shown in Figure 1C, a dose of 498.2 µM STC significantly decreased the viability of the AR42J cells; however, doses of 2.5, 5, 10, 20, and 40 µM emodin notably increased cells viability in a dose-dependent manner. Moreover, the morphology of AR42J cells was observed using a light microscope, and the results revealed that STC significantly caused AR42J cell death and morphological changes characteristic for cell death, which was alleviated by emodin at doses of 40, 20, and 10 µM (Figure 1D). Trypsin is a pancreatitis marker that can be assayed via a rhodamine staining kit (19). Using a confocal laser-scanning microscope, we identified trypsin-positive cells with green color, and emodin at doses of 40, 20, and 10 µM significantly decreased the number of trypsin-positive cells (Figure 1E). In addition, amylase is another common biochemical marker of pancreatic disease (28). Through ELISA, it found that STC significantly induced the release of amylase, which was decreased by emodin in a dose-dependent manner (Figure 1F). Moreover, the protein and gene levels of inflammatory mediators were all detected by ELISA and real-time PCR, respectively. The results showed that TNF-α, IL-1β, and IL-6 were markedly increased in AR42J cells after treatment with STC; however, they were notably decreased by emodin at both the gene and protein levels (Figures 1G,H). Thus, these results proved that emodin could alleviate STC-induced AR42J cell injury and inflammation.

In order to validate whether the HTRA1/TGF-β1 signaling pathway involves in the underlying mechanism of emodin against STC-induced AR42J cell injury, AR42J cells were treated with STC and different concentrations of emodin (40, 20, and 10 µM), and then the protein levels of HTRA1, TGF-β1, IL-33, MyD88, TRAF-6, and NF-κB were detected. The protein level of HTRA1 was significantly upregulated, and the protein level of TGF-β1 was markedly downregulated by STC compared with the control group; however, the alteration was reversed by emodin in a dose-dependent manner (Figures 2A,B). Subsequently, the levels of proteins downstream of the TGF-β1 inflammatory signal, including IL-33, MyD88, TRAF-6, and NF-κB, were all notably decreased by emodin compared to the STC-treated group. As previous method (29), the HTRA1 protein expression level was detected through the immunofluorescence assay, and the results indicated that STC notably increased the HTRA1 protein level (red fluorescence), which was markedly inhibited by emodin (40, 20, and 10 µM) in a dose-dependent manner (Figure 2C).

To explore the role of HTRA1 in the anti-inflammatory activity of emodin, an in vitro overexpression approach performed by HTRA1-pcDNA3.1 was used. As shown in Figure 3A, lipase and amylase levels in emodin-treated AR42J cells were significantly decreased compared with the STC group, but these inhibitory actions were significantly abrogated by HTRA1 overexpression regardless of the presence of emodin. Similar results were also observed at the protein and mRNA expression levels of TNF-α, IL-1β, and IL-6 (Figures 3B,C). In addition, as shown in Figures 3D,E, after transfecting with HTRA1-pcDNA3.1 regardless of the presence of emodin, the expression levels of HTRA1, IL-33, MyD88, TRAF-6, and NF-κB were all notably increased, and the TGF-β1 expression level was markedly decreased compared to the control group. These results suggested that overexpression of HTRA1 abrogated the regulation of the HTRA1/TGFβ1 signaling pathway by emodin.

Based on bioinformatic approaches, we collected the prospective target miRNAs of HTRA1 and predicted that miR-30a-5p might be an important transcriptional brake that modulates targeted HTRA1 mRNA translation. The RNA sequence alignment showed that the 3′-UTR of HTRA1 mRNA contained a site complementary to the seed region of miR-30a-5p (Figure S1 in Supplementary Material). To further verify this finding, dual luciferase reporter assay was performed, and the results showed that luciferase activity in HTRA1-WT plasmid group was significantly repressed by miR-30a-5p mimic, but the effect was not observed in the HTRA1-MUT plasmid group (Figure 4A). In addition, western blot analysis further showed that miR-30a-5p mimic could markedly downregulate HTRA1 protein expression in HTRA1-WT plasmid group (Figure 4B). Therefore, these results showed that miR-30a-5p was likely to control target HTRA1 gene expression, accordingly repressing protein translation. Furthermore, in order to determine whether emodin has a regulatory effect on miR-30a-5p, we detected the miR-30a-5p level through quantitative real-time PCR assay. As shown in Figure 4C, the results indicated that emodin at doses of 40, 20, and 10 µM significantly upregulated the expression levels of miR-30a-5p in AR42J cells compared with the model group. These results showed that the inhibition of emodin on HTRA1 maybe through activating miR-30a-5p expression.

To validate the inhibition of TGF-β1 by HTRA1, we constructed TGF-β1 promoter dual luciferase plasmid (TGF-β1-pGL3-Basic) and performed the dual luciferase reporter assay. As shown in Figure 4D, the results showed that HTRA1 overexpression could markedly decrease the relative luciferase activity compared to the negative control, indicating that the HTRA1 protein significantly inhibits the TGF-β1 protein. Moreover, to observe the effects of miR-30a-5p on the inhibition of TGF-β1 by HTRA1, the AR42J cells were transfected with miR-30a-5p mimic and inhibitor, respectively. The results showed that miR-30a-5p mimic increased the luciferase activity, which was decreased by miR-30a-5p inhibitor (Figure 4D). The underlying mechanism involves in the miR-30a-5p-mediated inhibition of HTRA1 protein. Therefore, these results further proved that miR-30a-5p targeted HTRA1 gene and affected the inhibition of TGF-β1 by HTRA1.

In vitro miR-30a-5p inhibitor transfection approach was used to observe the regulatory role of miR-30a-5p in the anti-inflammatory activity of emodin. The results showed that amylase and lipase levels were significantly increased by miR-30a-5p inhibitor both in the presence or absence of emodin compared with the control group; therefore, the inhibitory effects of emodin on lipase and amylase were significantly abrogated by miR-30a-5p inhibitor (Figure 5A). The protein and mRNA expression levels of TNF-α, IL-1β, and IL-6 in AR42J cells showed similar results (Figures 5B,C). Furthermore, after transfection of the cells with the miR-30a-5p inhibitor or miR-30a-5p inhibitor plus emodin, the expression levels of the HTRA1, IL-33, MyD88, TRAF-6, and NF-κB proteins were all significantly upregulated and the TGF-β1 protein level was markedly downregulated compared with the control group (Figures 5D,E). These results suggest that the miR-30a-5p inhibitor abrogated the protective effects of emodin on STC-injured AR42J cells and the regulation of the HTRA1/TGFβ1 signaling pathway by emodin.

To further explore the role of miR-30a-5p in protective effects of emodin against rat pancreatitis, in vivo miR-30a-5p antagomir experiment was performed according to the study schema (Figure 6A). As shown in Figure 6B, the amylase and lipase levels in emodin (60 mg·kg⁻¹)-treated rats were significantly decreased compared with the model rats, but these inhibitory actions were markedly abrogated in the miR-30a-5p antagomir group. Moreover, miR-30a-5p antagomir could markedly decrease the expression of miR-30a-5p regardless of the presence of emodin (Figure 6C). Furthermore, the histological architecture of pancreas tissue was investigated based on the HE staining (Figure 6D; Figure S2 in Supplementary Material). The results showed that pancreatic tissue injury of model group was characterized with acinar cell vacuolization, hemorrhage, leukocyte infiltration and necrosis; however, 60 mg·kg⁻¹ of emodin could markedly decrease these pathological changes, which were abrogated by the miR-30a-5p antagomir. Therefore, miR-30a-5p plays an important role in the protective effects of emodin against rat pancreatitis.

Myeloperoxidase is a classical biomarker of neutrophil activation and inflammation in pancreatitis (30). To examine the effects of emodin on HTRA1 expression and inflammation in pancreatic tissue, a double immunofluorescence assay was performed. As shown in Figure 6E, HTRA1 protein expression and the number of MPO-positive cells both significantly increased in the pancreatic tissue of rat pancreatitis compared with those in the control group, and this effect was decreased by emodin at a dose of 60 mg·kg⁻¹. Moreover, both in the presence or absence of emodin after transfecting with the miR-30a-5p antagomir, HTRA1 protein expression and the number of MPO-positive cells were notably increased, suggesting that the miR-30a-5p antagomir reversed the actions of emodin on HTRA1 expression and inflammation. Therefore, emodin primarily inhibited inflammatory reactions in vivo by increasing miR-30a-5p.

In order to test the role of miR-30a-5p in the regulation of inflammation and HTRA1/TGF-β1 signaling pathway by emodin in rat pancreatitis, in vivo miR-30a-5p antagomir experiment was performed. Similar results were also observed both on the TNF-α, IL-1β, and IL-6 plasma levels (Figure 7A) and the expression levels of TNF-α, IL-1β, and IL-6 mRNA in pancreas tissue (Figure 7B). Moreover, after transfecting with the miR-30a-5p antagomir, inflammatory factors including TNF-α, IL-1β, and IL-6 were significantly increased regardless of the presence of emodin, suggesting that the miR-30a-5p antagomir reversed the anti-inflammatory activity of emodin in model rats. In addition, as shown in Figures 7C,D, the protein expression levels of HTRA1, IL-33, MyD88, TRAF-6, and NF-κB were all notably decreased, and the TGF-β1 expression level was markedly increased after treatment with emodin (60 mg·kg⁻¹). However, these in vivo regulatory actions were all reversed by the miR-30a-5p antagomir. Therefore, miR-30a-5p silencing induced by its antagomir abrogated the anti-inflammatory activity of emodin in pancreatitis rats, which showed that miR-30a-5p exerted critical regulation in anti-inflammatory effect of emodin by regulating HTRA1/TGFβ1 signaling pathway.