The procedure and protocol for mesothelial cell culture have been detailed in our previous study (16). Met-5A mesothelial cells (cat. no. 65302), were obtained from Bioresource Collection and Research Center. This nonprofit organization, supported by the Taiwan government, upholds a strict quality control system, including sterility, mycoplasma contamination tests and short tandem repeat profiling analysis for each cell line. Met-5A cells were cultured in M199 medium (Gibco; Thermo Fisher Scientific, Inc.), supplemented with penicillin (100 U/ml) (Gibco; Thermo Fisher Scientific, Inc.), streptomycin (100 µg/ml) (Gibco; Thermo Fisher Scientific, Inc.) and 10% fetal bovine serum (Biowest), and were maintained at 37°C in a humidified atmosphere containing 95% air and 5% CO₂.

To assess the therapeutic effects of dulaglutide on protecting Met-5A cells from injury induced by p-Cresol (a uremic compound that serves as an oxidative stress inducer), cells were co-cultured with stepwise increasing doses of dulaglutide (0, 20, 50 and 100 µM; cat. no. PS1434; Eli Lilly and Company) and 50 µM p-Cresol (cat. no. 805223; Sigma-Aldrich; Merck KGaA) for 24 h at 37°C. Human Met-5A pleural mesothelial cells were used in vitro and were divided into five groups: i) A1, Met-5A cells only; ii) A2, Met-5A cells + 50 µM p-Cresol, cultured for 24 h; iii) A3, Met-5A cells + 50 µM p-Cresol + 20 µM dulaglutide, co-cultured for 24 h; iv) A4, Met-5A cells + 50 µM -Cresol + 50 µM dulaglutide, co-cultured for 24 h; and v) A5, Met-5A cells + 50 µM p-Cresol + 100 µM dulaglutide, co-cultured for 24 h. The concentrations of p-Cresol (35) and dulaglutide (36) were selected based on our previous reports, with slight modifications: 50 µM p-Cresol, and 0, 20, 50 and 100 µM dulaglutide were used.

To determine whether a 100 µM dosage of dulaglutide adequately protected cell viability and prevented apoptosis under p-Cresol stimulation, the Met-5A cell line was divided into three groups: B1, Met-5A cells only; B2, Met-5A cells cultured with 50 µM p-Cresol; and B3, Met-5A cells co-cultured with 50 µM p-Cresol and 100 µM dulaglutide. Cells were collected at 24, 48 and 72 h for MTT assay. In addition, cells harvested at 72 h were subjected to flow cytometric analysis to evaluate intracellular reactive oxygen species (ROS) generation as well as early and late apoptotic events.

To assess the therapeutic impact of dulaglutide on the expression of inflammatory markers by western blotting, Met-5A cells were used in vitro and were divided into the following groups: C1, Met-5A cells only; C2, Met-5A cells + 10 µg/ml LPS (cat. no. L2880; Sigma-Aldrich; Merck KGaA), cultured for 12 h; and C3, Met-5A cells pretreated with 100 µM dulaglutide for 12 h, followed by the addition of 10 µg/ml LPS and further culture for 12 h, totaling 24 h. Inflammatory responses were evaluated by detecting the expression levels of Toll-like receptor (TLR)-2, TLR-4, NF-κB, TNF-α and MMP-9 via western blot analysis, and CD11b⁺ cells were observed under a fluorescence microscope. The dosage of LPS (10 µg/ml) was based on our previous report (33).

To examine the roles of TGF-β and DPP4 in the development of EMT and PF, the Met-5A cell line was divided into the following groups: D1, Met-5A cells only; D2, Met-5A cells + 50 µM p-Cresol, cultured for 24 h; D3, double knockdown of TGF-β and DPP4 genes in Met-5A cells for 24 h; D4, Met-5A cells + double knockdown of TGF-β and DPP4 genes for 24 h, followed by treatment with 50 µM p-Cresol for an additional 24 h. For double knockdown of the TGF-β and DPP4 genes, the TGF-β, DPP4 and negative control small interfering (si)RNAs were used. The sequences were as follows: siRNA1-TGF-β, sense 5′-GGA GAG CCC UGG AUA CCA ATT-3′, antisense, 5′-UUG GUA UCC AGG GCU CUC CGG-3′ (cat. no. S133088; Thermo Fisher Scientific, Inc.); siRNA2-TGF-β, sense 5′-GCA ACA ACG CAA UCU AUG ATT-3′, antisense 5′-UCA UAG AUU GCG UUG UUG CGG-3′ (cat. no. S133090; Thermo Fisher Scientific, Inc.); siRNA1-DPP4, sense 5′-GCG UGA AUG AUA AAG GGC UTT-3′, antisense 5′-AGC CCU UUA UCA UUC ACG CTG-3′ (cat. no. S4254; Thermo Fisher Scientific, Inc.); siRNA2DPP4, sense 5′-GGU CAC CAG UGG GUC AUA ATT-3′, antisense 5′-UUA UGA CCC ACU GGU GAC CAT-3′ (cat. no. S4256; Thermo Fisher Scientific, Inc.). For efficient knockdown of the TGF-β and DPP4 genes, pooled siRNAs (siRNA1 and siRNA2) targeting each gene were used. For TGF-β knockdown, siRNA1-TGF-β and siRNA2-TGF-β were combined. Similarly, DPP4 knockdown was achieved using a combination of siRNA1-DPP4 and siRNA2-DPP4. The negative control siRNA was purchased from Santa Cruz Biotechnology, Inc. (scrambled siRNA control; cat. no. sc-37007). In the present study, the transient transfection of siRNAs was conducted using GenMute™ siRNA Transfection Reagent (cat. no. SL100568; SignaGen Laboratories) according to the manufacturer's instructions. Briefly, Met-5A cells at a density of ~1×10⁶ cells were cultured to 50% confluence in 10-cm plates and were transfected with 5 µM siRNA-TGF-β, siRNA-DPP4 or negative control siRNA at 37°C for 24 h. Following 24 h of transfection, Met-5A cells were treated with 50 µM p-Cresol or harvested for further experiments.

For the MTT assay, 5,000 cells/well were plated in a 96-well plate. After an overnight incubation, the cells were treated with p-Cresol or dulaglutide for 1, 2 or 3 days. At the indicated time, the culture medium was removed, followed by the addition of 200 µl MTT reagent. After further incubation for 30 min, the reagent was removed, and the cells were solubilized with 100 µl DMSO. A spectrophotometer was used to record the optical density at 595 nm.

Given that injury to peritoneal tissues can induce a transition of mesothelial cells to a mesenchymal phenotype through EMT, a cellular model was generated to investigate whether dulaglutide could inhibit this transition. The Met-5A cells were categorized into the following groups: E1, Met-5A cells only; E2, Met-5A cells + 3 ng/ml TGF-β1 (cat. no. 240-B; R&D Systems, Inc.) + 10 ng/ml epithelial growth factor (EGF; cat. no. AF-100-15; Peprotech; Thermo Fisher Scientific, Inc.), co-cultured for 5 days; E3, Met-5A cells + 5.0 µM CG (cat. no. GMP G-10846; Panion & BF Biotech Inc.), cultured for 5 days; E4, Met-5A cells + TGF-β1 + 10 ng/ml EGF + dulaglutide, co-cultured for 5 days; E5, Met-5A cells + CG + dulaglutide, co-cultured for 5 days. The dosages of TGF-β1, EGF and the culturing times were based on a previous report (16), with some modifications: 3 ng/ml TGF-β1 and 10 ng/ml EGF were used for 5 days at 37°C. TGF-β1 was used as a positive control for EMT. Cell morphology was subsequently observed under a fluorescence microscope (Olympus BX53; Olympus Corporation) at ×200 magnification.

Prior to surgical procedures, an anesthesia box was pre-charged with 5% isoflurane for 5 min to fully saturate the atmosphere. Once the rat was placed inside, the concentration was reduced to 3% until the respiratory rate stabilized, then maintained at 2% throughout the surgical procedure. At the conclusion of the surgery, while preparing for suturing, the isoflurane level was reduced to 1%.

To determine whether dulaglutide therapy can protect rat PF against CG injury, the procedures and protocols from our recent report (16) were adapted, with the following modifications. Specifically, pathogen-free adult male Sprague-Dawley rats (Charles River Laboratories, Inc.), weighing 300-325 g and aged 70-75 days were used in the present study. All animal procedures were approved by the Institute of Animal Care and Use Committee at Kaohsiung Chang Gung Memorial Hospital (Affidavit of Approval of Animal Use Protocol No. 2021080501) and were performed in accordance with the Guide for the Care and Use of Laboratory Animals (37). Animals were housed in an Association for Assessment and Accreditation of Laboratory Animal Care International-approved animal facility in the hospital with controlled humidity (55±10%), temperature (24°C) and light cycles (12-h light/dark cycle). Rats had free access to standard laboratory chow and autoclaved drinking water throughout the study. A total of 24 rats were randomly assigned into four groups (n=6/group) for experimental analysis. PF was induced through daily intraperitoneal injections of 0.1% CG in saline at a dose of 10 ml/kg body weight into the peritoneal cavity for 21 consecutive days. This experimental model of PF has been described in our previous report (16). The sham control (SC) group received an equal amount of 0.9% saline. Additionally, dulaglutide (10 µg/kg; cat. no. PS1434; Eli Lilly and Company) was administered subcutaneously to rats weekly for 3 weeks starting 1 week after the initial CG injection to evaluate early treatment effects aimed at preventing PF. The dosage of dulaglutide (10 µg/kg) was based on our previous studies (34,36) with some modifications-, dulaglutide (10 µg/kg) was used here as a GLP-1 receptor agonist.

The rats were divided into the following four groups: i) SC group, receiving only normal saline injections; ii) CKD group; iii) CKD + CG group, with PF induced by CG; and iv) CKD + CG + dulaglutide group, PF was induced by CG and rats received weekly subcutaneous injections of 10 µg/kg dulaglutide for 3 consecutive weeks, starting on day 21 after CKD induction. Notably, it is not possible to create an animal model of ESRD due to the high mortality and rapid progression to uremia, which compromise long-term survival and experimental control. Instead, a model of CKD was developed, which simulates conditions similar to ESRD. Moreover, PF induction was initiated on day 14 following CKD induction.

The procedure and protocol for CKD induction have been detailed in our previous report (38). Briefly, all rats were anesthetized with 2.0% isoflurane via inhalation, placed supine on a warming pad at 37°C and underwent midline laparotomies. The SC rats underwent laparotomy only, whereas CKD was induced in the CKD groups by right nephrectomy and arterial ligation of the upper two-thirds (upper and middle poles) of the blood supply to the left kidney, preserving only the lower third (lower pole) with normal blood supply. This model preserves a limited amount of functioning renal parenchyma to simulate CKD.

Blood samples (1 ml) were serially collected via the lateral tail vein before and after the CKD induction (i.e., prior to and at days 14, 35 and 42 before euthanasia) to evaluate the creation of the CKD model and the therapeutic impact of dulaglutide on protecting residual renal function and suppressing the PF process. Serum levels of creatinine and BUN, and circulating levels of DPP4 and GLP-1, as well as peritoneal fluid levels of GLP-1 and DPP4, were measured in duplicate using standard laboratory equipment. Immediately after sacrifice and prior to abdominal dissection, 10 ml sterile, pre-warmed PBS was gently injected into the peritoneal cavity using a sterile syringe. The abdomen was lightly massaged for 30 sec to distribute the fluid, after which, a second syringe was used to aspirate the peritoneal lavage fluid, typically recovering 5-8 ml/rat. The fluid was centrifuged at 200 × g for 10 min at 4°C to remove cells and debris, and the supernatant was collected and detecttored at −80 °C. Detection of DPP4 (cat. no. ab204722; Abcam) and GLP-1 (cat. no. EGLP-35K; MilliporeSigma) were measured in duplicate using ELISA kits according to the manufacturers' instructions.

The procedure for 24-h urine collection is described in our previous report (38). For this study, each rat was placed in a metabolic cage (DXL-D; dimensions: 190×290×550 mm³; Suzhou Fengshi Laboratory Animal Equipment Co., Ltd.) for 24 h with free access to food and water. Urine was collected over 24 h prior to and at days 14, 35 and 42 after CKD induction to determine the ratio of urine protein to creatinine. Urine samples were centrifuged at 380 × g for 10 min at 4°C to remove particulate matter, and the samples were aliquoted and stored at -80°C until biochemical analysis. Urinary protein levels were measured using a bicinchoninic acid (BCA) protein assay kit (cat. no. 23225; Thermo Fisher Scientific, Inc.). Urinary creatinine was measured using the Creatinine Assay Kit-Colorimetric (cat. no. ab65340; Abcam). Assays were performed according to the manufacturers' instructions,

To evaluate intracellular ROS generation, mitochondrial ROS levels and apoptotic cell death in Met-5A cells (groups B1, B2 and B3), cells were collected at 72 h, washed with PBS, and stained with DCFDA (cat. no. ab113851; Abcam) for 30 min, mitoSOX (cat. no. M36008; Invitrogen; Thermo Fisher Scientific, Inc.) for 15 min, and Annexin V-FITC and PI (cat. no. 556547; BD Pharmingen; BD Biosciences) for 30 min at 37°C. To identify and characterize neutrophils and myeloid-derived inflammatory cells in circulating blood and abdominal fluid, samples were collected from experimental animals and stained with CD11b/c-PE (cat. no. 554862; BD Pharmingen; BD Biosciences), Ly6g-FITC (cat. no. ab25024; Abcam) and intracellular myeloperoxidase (MPO)-FITC (cat. no. ab90812; Abcam) for 30 min at 4°C. Cell suspensions were washed with PBS and then analyzed on a flow cytometer. Flow cytometric analysis was performed at the Translational Research Center, Kaohsiung Chang Gung Memorial Hospital (Kaohsiung, Taiwan) using a BD FACSCanto™ II flow cytometer (BD Pharmingen; BD Biosciences). Data were acquired with BD FACSDiva™ Software, version 8.0.1 (BD Pharmingen; BD Biosciences) and analyzed using FlowJo™ Software, version 10.8.1 (BD Pharmingen; BD Biosciences).

To assess the impact of peritoneal inflammatory reactions on inducing mesothelial cell damage and subsequent PF, 18 additional Sprague-Dawley rats were divided into the following three groups (n=6/group): i) SC group, receiving normal saline; ii) LPS-induced peritonitis group, rats received a single intra-peritoneal injection of 3.8% glucose (2.0 ml) and peritonitis was induced through a single intraperitoneal administration of LPS (1.5 mg/kg); and iii) peritonitis + dulaglutide group, rats received glucose and peritonitis was induced through intraperitoneal administration of LPS, with a pre- and post-induction subcutaneous injection of 10 µg/kg dulaglutide 3 days prior to and 1 day after peritonitis induction.

The rats were euthanized on day 5, which was defined as the acute phase of peritonitis. Prior to euthanasia, a catheter was inserted into the jugular vein, and the abdomen was opened. Peritoneal fluid was aspirated and replaced with 1 ml 3.33 M FITC-dextran 10000 (Sigma-Aldrich; Merck KgaA). All rats were anesthetized with 2.0% isoflurane via inhalation and blood samples (1 ml) were drawn from the jugular vein at intervals of 10, 20 and 30 min to measure the concentration of FITC-dextran. After collecting the final blood sample, the rats were euthanized by exsanguination under deep anesthesia. The procedure and protocol for testing the leakage of FITC-dextran from circulation into the peritoneum were based on our previous study with the following modifications (39). Plasma samples collected at each time point were centrifuged at 1,000 × g for 10 min at 4°C to remove cellular debris. The supernatants were collected and transferred to a black 96-well plate to determine the concentration of FITC-dextran using a fluorescence microplate reader (SpectraMax; Molecular Devices, LLC) with an excitation wavelength of 485 nm and an emission wavelength of 530 nm. All measurements were performed in triplicate.

At day 42 post-CKD induction, all rats-including those in SC, CKD, CKD + CG and CKD + CG + dulaglutide groups, were euthanized under the same conditions to ensure consistency in tissue sampling and data comparison. Rats were deeply anesthetized with 2.0% isoflurane, and euthanasia was performed by exsanguination via terminal blood collection (>10 ml) under anesthesia. This procedure typically required ~5 min, during which 2.0% isoflurane inhalation was maintained. Following respiratory arrest, the kidneys and peritoneum were harvested for histopathological analysis.

The histopathological scoring of kidney injury was conducted in a blinded fashion as described in our previous report (40). Briefly, left kidney specimens from all rats were fixed in 10% buffered formalin for 24 h at 25°C, embedded in paraffin, and sectioned at 4 µm. Sections were deparaffinized, rehydrated, and stained with hematoxylin for 5 min and eosin for 2 min. After dehydration and mounting, sections were evaluated by light microscopy evaluation. The injury was scored based on the grading of tubular necrosis, loss of brush border, cast formation and tubular dilatation across 10 randomly selected, non-overlapping fields (×200 magnification) for each animal as follows: 0 (none), 1 (≤10%), 2 (11-25%), 3 (26-45%), 4 (46-75%) and 5 (≥76%).

The procedure and protocol for western blotting have been described in our previous reports (41-46). Kidney tissues or cells were lysed in M-PER™ (cat. no. 78501; Thermo Fisher Scientific, Inc.) containing protease (cat. no. 539134; Sigma-Aldrich; Merck KGaA) and phosphatase inhibitor cocktails (cat. no. 524629; Sigma-Aldrich; Merck KGaA). Protein concentration was determined using the BCA assay (Pierce™ BCA Protein Assay Kit; cat. no. 23225; Thermo Fisher Scientific, Inc.), following the manufacturer's instructions, with bovine serum albumin (BSA) (cat. no. A9418; Sigma-Aldrich; Merck KgaA) as a standard. Equal amounts (50 µg) of protein extracts were loaded and separated by SDS-PAGE on 12% gels using acrylamide gradients. After electrophoresis, the proteins were transferred electrophoretically to polyvinylidene difluoride membranes (Amersham; Cytiva). Non-specific binding was blocked by incubating the membranes in blocking buffer (5% non-fat dry milk in TBS containing 0.05% Tween 20) overnight at 4°C. Primary antibodies used in the western blot analysis included: NOX-1 (1:1,000; cat. no. SAB4200097; Sigma-Aldrich; Merck KGaA), NOX-2 (1:1,000; cat. no. MABS2195; Sigma-Aldrich; Merck KGaA), TNF-α (1:1,000; cat. no. 3707; Cell Signaling Technology, Inc.), IL-1α (1:1,000; cat. no. 84618; Cell Signaling Technology, Inc.), MMP-9 (1:1,000; cat. no. ab76003; Abcam), DPP4 (1:1,000; cat. no. ARP63319_P050; Aviva Systems Biology), phosphorylated (p)-Smad3 (1:1,000; cat. no. 9520; Cell Signaling Technology, Inc.), Smad3 (1:1,000; cat. no. 9513; Cell Signaling Technology, Inc.), TGF-β (1:3,000; cat. no. ab215715; Abcam), GLP-1 (1:1,000; cat. no. ab108443; Abcam), GLP-1R (1:1,000; cat. no. ab218532; Abcam), nuclear factor erythroid 2-related factor 2 (Nrf2; 1:1,000; cat. no. ab62352; Abcam), NAD(P)H quinone oxidoreductase 1 (NQO-1; 1:1,000; cat. no. ab80588; Abcam), Snail (1:1,000; cat. no. 3879; Cell Signaling Technology, Inc.), von Willebrand factor (vWF; 1:1,000; cat. no. ab154193; Abcam), VEGF (1:1,000; cat. no. ab214424; Abcam), α-smooth muscle actin (α-SMA; 1:6,000; cat. no. A2547; Sigma-Aldrich; Merck KGaA), vimentin (1:1,000; cat. no. 5741; Cell Signaling Technology, Inc.), β-catenin (1:1,000; cat. no. 8480; Cell Signaling Technology, Inc.), fibronectin (1:1,000 cat. no. ab2413; Abcam), collagen I (1:1,000; cat. no. C2456; Sigma-Aldrich; Merck KGaA), N-cadherin (1:1,000; cat. no. 13116; Cell signaling Technology, Inc.), TLR-2 (1:4,000; cat. no. ab213676; Abcam), TLR-4 (1:4,000; cat. no. NB100-56566; Novus Biologicals, LLC; Bio-Techne), NF-κB (1:1,000; cat. no. 8242; Cell Signaling Technology, Inc.), p-NF-κB (1:1,000; cat. no. 3033; Cell Signaling Technology, Inc.), CD31 (1:1,000; cat. no. 77699; Cell Signaling Technology, Inc.) and β-actin (1:10,000; cat. no. A5441; MilliporeSigma). The membranes were then incubated with the indicated primary antibodies for 1 h at room temperature, followed by a horseradish peroxidase-conjugated anti-rabbit (1:3,000; cat. no. A0545; MilliporeSigma) or anti-mouse immunoglobulin IgG (1:3,000; cat. no. A5278; MilliporeSigma) for 1 h at room temperature. The washing procedure was repeated eight times within 1 h. Immunoreactive bands were visualized using enhanced chemiluminescence (Amersham; Cytiva) and exposed to Biomax L film (Kodak). For semi-quantification purposes, ECL signals were digitized using Labwork software (version 4.6; Analytik Jena AG).

The procedures and protocols for IF studies were based on our previous reports (40-46). Kidney and peritoneum tissues were fixed in 10% neutral-buffered formalin at room temperature (25°C) for 24 h, embedded in paraffin and cut into 4-µm sections using a rotary microtome. Sections were then deparaffinized in xylene and rehydrated through a graded ethanol series. Citrate buffer (10 mM, pH 6.0) was used to perform antigen retrieval in a microwave for 15 min and sections were incubated in 5% BSA in PBS for 1 h at room temperature (22-25°C) to block non-specific binding. Sections were then incubated overnight at 4°C with rabbit anti-MMP-9 antibody (1:200; cat. no. MA5-14228; Invitrogen; Thermo Fisher Scientific, Inc.) or IgG Isotype Control (1:200, cat. no. 02-6102; Invitrogen; Thermo Fisher Scientific, Inc.). After washing with PBS, the sections were incubated with goat anti-rabbit IgG (H+L) Alexa Fluor^® 488-conjugated secondary antibody (1:500; cat. no. A-11008; Invitrogen; Thermo Fisher Scientific, Inc.) for 1 h at room temperature in the dark. Sections were counterstained with DAPI (1 µg/ml) for 5 min, rinsed and mounted with antifade mounting medium. For semi-quantification, three randomly selected high-power fields (HPFs) at ×200 magnification were evaluated in each section under a fluorescence microscope (Olympus BX53; Olympus Corporation). The mean number per HPF for each animal was determined by summing all counts and dividing by 9. Furthermore, tissue slides were reviewed by an expert in rodent pathology.

For IF staining of cultured cells, the cells were cultured on sterile glass coverslips in 12-well plates. After treatment, the cells were rinsed with PBS, fixed with 4% paraformaldehyde in PBS for 15 min at 22-25°C, then permeabilized with 0.1% Triton X-100 in PBS for 10 min at room temperature. Non-specific binding was blocked using 5% BSA in PBS for 1 h at room temperature. Cells were incubated overnight at 4°C with anti-CD11b (1:200; cat. no. 114-0118-82; Invitrogen; Thermo Fisher Scientific, Inc.), and after washing with PBS twice, they were incubated for 1 h at 4°C with Goat anti-mouse IgG (H+L), Alexa Fluor 488 (1:500; cat. no. A-11008; Invitrogen; Thermo Fisher Scientific, Inc.). For phalloidin staining, the cells were incubated 1 h at 4°C with Phalloidin-iFluor 488 (1:400; cat. no. ab176753; Abcam). Subsequently, the cells were counterstained with DAPI for 5 min, rinsed, mounted with antifade mounting medium and observed under a fluorescence microscope (Olympus BX53; Olympus Corporation).

For Masson's staining, paraffin-embedded peritoneal tissue sections (4 µm) were deparaffinized, rehydrated and subjected to Masson's trichrome staining using a standard protocol (Masson's Trichrome Stain Kit; cat. no. 87019; Thermo Fisher Scientific, Inc.). Briefly, sections were fixed in Bouin's solution at 56°C for 1 h to enhance staining, followed by staining with Weigert's iron hematoxylin for nuclei at room temperature for 10 min, Biebrich scarlet-acid fuchsin for cytoplasm and muscle fibers at room temperature for 10 min, and aniline blue for collagen at room temperature for 5 min. Slides were then differentiated in phosphomolybdic-phosphotungstic acid, dehydrated through graded ethanol, cleared in xylene and mounted. The extent of fibrosis was evaluated under a light microscope and was semi-quantified using ImageJ software (version 1.51; National Institutes of Health).

Quantitative data are presented as the mean ± SD. Statistical analyses were conducted using SAS statistical software, version 8.2 (SAS Institute, Inc.). One-way ANOVA followed by Bonferroni's multiple comparisons post hoc test was used to compare variables among groups. Additionally, kidney injury scores were presented as the median (interquartile range), and were analyzed using Kruskal-Wallis test and Dunn's post hoc test. P<0.05 was considered to indicate a statistically significant difference.

It is well-known that uremic toxic substances frequently induce oxidative stress and inflammatory reactions (47). To assess the impact of dulaglutide on suppressing these detrimental signaling pathways, the Met-5A cell line was split into five groups, and western blot analysis was conducted. The results showed that the protein expression levels of NOX-1 and NOX-2 (Fig. S1A, B and E), indicators of oxidative stress, and TNF-α, IL-1β and MMP-9 (Fig. S1A, F, H and I), markers of inflammation, were significantly higher in A2 compared with in A1. Notably, the levels of these markers were significantly and progressively reversed in groups A3-A5, suggesting that dulaglutide may effectively suppress uremic toxic substance-induced oxidative stress and inflammation, particularly at higher dosages.

Additionally, the protein expression levels of DPP4 (Fig. S1A and J), a marker of hyperglycemia and insulin sensitivity suppression, and p-Smad3/Smad3 and TGF-β (Fig. S1A, D and G), indicators of fibrosis, exhibited a similar pattern. Conversely, the protein expression levels of GLP-1 and GLP-1R (Fig. S1A, C and L), which promote insulin secretion displayed an opposite pattern to oxidative stress markers among the groups. The antioxidants Nrf2 and NQO-1 (Fig. S1A, K and M) were significantly higher in A5 and progressively decreased in groups A2-A4 compared with in A1.

Next, the present study aimed to determine whether a 100 µM concentration of dulaglutide (i.e., the highest dose utilized in Fig. S1) was safe for the cell culture study. The cell line was divided into groups B1-B3, and the MTT assay and flow cytometric analysis were conducted. The results showed that cell viability was significantly lower in B2 cells compared with that in the B1 group, but that it was significantly reversed in the B3 group at 24, 48 and 72 h (Fig. S2A-C). Additionally, after 72 h, total intracellular (Fig. S2D and E) and mitochondrial (Fig. S2F and G) ROS levels, along with early (Annexin-V⁺/PI⁻) and late (Annexin-V⁺/PI⁺) apoptosis (Fig. S2H-J) in Met-5A cells, were significantly higher in the B2 group than in the B1 and B3 groups, but were significantly higher in the B3 group than in the B1 group. These findings suggested that 100 µM dulaglutide not only provided adequate cell protection against ROS levels and apoptosis but also was not harmful to the Met-5A cells. Accordingly, 100 µM dulaglutide was utilized in the subsequent in vitro study.

Previous studies have demonstrated that GLP-1 antagonists protect renal function from inflammation and oxidative stress-induced kidney damage in settings of acute kidney injury (48,49) and CKD, mainly through the suppression of DPP4 activity (16). To verify the therapeutic impact of dulaglutide on attenuating the LPS-induced inflammatory reaction, mimicking the clinical setting of endotoxin-mediated peritonitis, Met-5A cells were used. The results of western blotting showed that the protein expression levels of TLR-2, TLR-4, NF-κB, TNF-α and MMP-9 were significantly higher in group C2 compared with those in group C1, but were significantly reversed in group C3 (Fig. S3A-F). Additionally, IF analysis revealed that the positively stained CD11b surface marker in Met-5A cells was markedly increased in group C2 compared with in group C1, consistent with enhanced inflammatory response (Fig. S3G-J), suggesting that dulaglutide may effectively suppress endotoxin-induced peritonitis in patients undergoing PD.

To verify whether the knockdown of TGF-β and DPP4 genes was specific, western blotting was performed to examine protein levels. The results confirmed successful transfection, as the expression levels of TGF-β and DPP4 were markedly reduced in the knockdown group compared with those in the control and negative control groups. The results also showed that transfection alone did not alter the protein levels of EMT-, oxidative stress-, or inflammation-related biomarkers compared with those in the control and negative control groups (Fig. S4).

Our previous studies have established the association between the EMT process and lung and kidney fibrosis (16,41). The present study aimed to elucidate whether DPP4 and TGF-β serve crucial roles in regulating the EMT process and tissue fibrosis, which can result in PF and, ultimately, PD failure. An in vitro study was conducted using western blot analysis. The protein expression levels of TGF-β (Fig. S5A and G) and p-Smad3 (Fig. S5A and F), indicators of fibrosis; Snail (Fig. S5A and I), α-SMA (Fig. S5A and J), vimentin (Fig. S5A and C) and β-catenin (Fig. S5A and K), markers of EMT; NOX-1 (Fig. S5A and L) and NOX-2 (Fig. S5A and D), indicators of oxidative stress; and NF-κB (Fig. S5A and E) and TNF-α (Fig. S5A and M), markers of inflammation, were significantly higher in group D2 compared with those in D1. The efficiency of the double knockdown was confirmed by markedly reduced protein expression levels of both TGF-β and DPP4 (Fig. S4). Notably, the levels of these markers were significantly reversed in the D3 group, which underwent successful double silencing of TGF-β and DPP4, but were then upregulated in group D4. By contrast, the protein expression levels of GLP-1 (Fig. S5A and B) displayed an opposite trend to the aforementioned markers. These findings indicated that these two genes may have key roles in EMT and PF.

Based on the aforementioned findings, the current study aimed to determine whether dulaglutide could suppress the upregulation of EMT biomarkers induced by TGF-β1 and CG in the Met-5A cell line. After culturing for 5 days, cells were collected for western blot analysis. The results showed that the protein expression levels of p-Smad3 (Fig. S6A and B), TGF-β (Fig. S6A and E), Snail (Fig. S6A and C), α-SMA (Fig. S6A and G), vimentin (Fig. S6A and D), β-catenin (Fig. S6A and F) and fibronectin (Fig. S6A and H), which are key EMT markers, were lowest in group E1, highest in group E2, and significantly higher in group E3 than in groups E4 and E5, with levels in E4 also being significantly higher than those in E5. These findings suggested that dulaglutide treatment may effectively inhibit the EMT process.

To elucidate the morphological features of the cytoskeleton in Met-5A cells, which can be used as indicators of the EMT process, the cells were divided into groups E1-E5, and IF staining was performed. The aim of this experiment was to determine whether dulaglutide could counteract CG-induced EMT-like cytoskeletal changes in Met-5A cells. The results demonstrated that the cytoskeleton (Fig. S7A-E) not only appeared more crowded in groups E2 and E3, but also exhibited a more typical mesenchymal cell morphology, with spindle-shaped features (Fig. S7G). Additionally, significant increases in cell length (Fig. S7F) and the mean fluorescence intensity of phalloidin staining (Fig. S7H) were observed in groups E2 and E3 compared with those in groups E1, E4 and E5. These elevated cell length and fluorescence intensity values were also significantly higher in groups E4 and E5 compared with those in group E1. This attenuation of EMT-associated cytoskeletal remodeling in the presence of dulaglutide further suggests that dulaglutide treatment significantly suppressed the EMT process in CG-treated renal tubular epithelial cells.

To assess the protective effects of dulaglutide against CKD-induced kidney damage and its impact on DPP4 activity, time-course blood sampling, biochemical examinations and ELISA were conducted in an in vivo study (Figs. 1 and S8). The experimental groups were as follows: SC, CKD, CKD + CG and CKD + CG + dulaglutide. The baseline serum levels of BUN (Fig. 1A), creatinine (Fig. 1B), DPP4 (Fig. 1C), GLP-1 (Fig. 1D) and R^Up/c (Fig. 1E) showed no significant differences among the groups. However, by day 14 post-CKD induction, the circulating levels of BUN (Fig. 1F), creatinine (Fig. 1G) and R^Up/c (Fig. 1J) were markedly lower in the SC group than in groups CKD, CKD + CG and CKD + CG + dulaglutide, with no differences noted among the latter three groups. Additionally, ELISA results indicated that the circulating levels of DPP4 (Fig. 1H) were markedly lower in the SC group than those in groups CKD, CKD + CG and CKD + CG + dulaglutide, and l with no difference between groups CKD + CG and CKD + CG + dulaglutide. Conversely, the circulating levels of GLP-1 (Fig. 1I) exhibited an opposite pattern to DPP4 among the groups.

Post-CKD induction, the circulating levels of creatinine on day 35 (Fig. 1L) and DPP4 on days 35 and 42 (Fig. 1M and R) were highest in the CKD + CG groups, lowest in the SC group, and significantly lower in the CKD + CG + dulaglutide group than in the CKD group, whereas the circulatory level of GLP-1 displayed an opposite pattern to DPP4 among the groups (Fig. 1N and S). However, the circulating levels of creatinine on day 42 (Fig. 1Q) were highest in the CKD groups, lowest in the SC group, and significantly lower in the CKD + CG + dulaglutide group than in the CKD + CG group. Furthermore, on days 35 and 42 post-CKD induction, BUN (Fig. 1K and P) and R^Up/c (Fig. 1O and T) were highest in the CKD group and lowest in the SC group.

To explore the impact of PF on the upregulation of EMT biomarkers and the mitigating effects of dulaglutide treatment, western blot analysis was utilized in the present study. As anticipated, the protein expression levels of the EMT biomarkers TGF-β (Fig. 2A and B), Snail (Fig. 2A and C), β-catenin (Fig. 2A and D), p-Smad3/Smad3 (Fig. 2A and E), vimentin (Fig. 2A and F), α-SMA (Fig. 2A and G), collagen I (Fig. 2A and H), N-cadherin (Fig. 2A and I) and fibronectin (Fig. 2A and J) were highest in the CKD + CG group, lowest in the SC group, and significantly lower in the CKD + CG + dulaglutide group than in the CKD group. These findings suggested that PF augmented the expression levels of EMT biomarkers, which were markedly suppressed by dulaglutide treatment.

Subsequently, the present study aimed to examine the effects of PF and dulaglutide therapy on the regulation of molecular markers in the rat peritoneum using western blot analysis. The results indicated that the protein expression levels of NOX-1 (Fig. 3A and B) and NOX-2 (Fig. 3A and E), markers of oxidative stress; and p-NF-κB (Fig. 3A and I) and TNF-α (Fig. 3A and F), markers of inflammation; and VEGF (Fig. 3A and L), an angiogenic factor, were lowest in the SC group, highest in the the CKD + CG group, and significantly lower in the CKD + CG + dulaglutide group than in the CKD group. Similarly, the protein expression levels of CD31 (Fig. 3A and J) and vWF (Fig. 3A and C), which are indicators of angiogenesis and endothelial function, and DPP4 (Fig. 3A and K), which is involved in oxidative stress, exhibited similar trends.

By contrast, the protein expression levels of GLP-1R (Fig. 3A and D), Nrf2 (Fig. 3A and G) and NQO-1 (Fig. 3A and H), markers of an antioxidative response, exhibited a pattern opposite to that of oxidative stress markers among the groups. These findings suggested that dulaglutide therapy could markedly suppress oxidative stress and abnormal angio-genesis in the peritoneum.

To explore the ultrastructural features of the peritoneum, microscopy was employed to identify histopathological changes in the rat peritoneum (Fig. 4A-D) following the induction of CKD, using hematoxylin and eosin staining. The results showed that the thickness (Fig. 4E) and hyperplasia (Fig. 4F) of the parietal layer of the peritoneum, both indicators of peritoneal proliferation, and the number of vessels (defined as ≤25 µm) (Fig. 4G) were highest in the CKD + CG group than in the other groups, higher in the CKD group than the SC and CKD + CG + dulaglutide groups, and were moderately higher in the CKD + CG + dulaglutide group than in the SC group. Furthermore, the number of muscularized vessels (Fig. 4H) in the parietal layer exhibited a similar pattern to that of small vessels among the groups, except it was similar between groups CKD and CKD + CG. The histopathological findings confirmed the successful creation of a PF model in CKD rats that mimics the clinical setting of PF in patients undergoing PD. These findings suggested that GLP-1 analogs may have potential clinical use in patients undergoing PD to prevent PD failure.

Moreover, Masson's trichrome and IF staining were used to verify the changes in fibrosis and inflammatory cell infiltration in the peritoneum following CG stimulation and dulaglutide therapy. The results revealed that the fibrotic area (Fig. 5A-E) and MMP-9 cell infiltration (Fig. 5F-J), an index of inflammation, in the parietal layer of the peritoneum were lowest in the SC group 1, highest in the CKD + CG group, and significantly lower in the CKD + CG + dulaglutide group than in the CKD group. These findings indicated that dulaglutide therapy may be promising for clinical use in patients undergoing PD to prevent PF and inflammation.

Additionally, light microscopy was used to evaluate the microstructural features of damaged kidney parenchyma and the morphology of the peritoneum in CKD rats in detail. The results showed that the kidney injury score (Fig. 6A-E) and the levels of MMP-9⁺ cells (Fig. 6F-J) in the kidney parenchyma were significantly increased in the CKD group and further increased in the CKD + CG group compared with those in the SC group, but were significantly reversed in the CKD + CG + dulaglutidegroup. These findings suggested that dulaglutide therapy not only mitigated inflammatory cell infiltration but also protected the kidney parenchyma against damage from CKD-related uremic toxins.

To determine whether inflammation serves a central role in peritoneal damage, an additional 24 animals were divided into the following groups: SC group, peritonitis induced by LPS group, and peritonitis induced by LPS + dulaglutide group, as aforementioned. As expected, the circulatory levels of GLP-1 (Fig. 7A) and DPP4 (Fig. 7B) at baseline did not differ among the three groups. However, by day 5 after the induction of peritonitis, ELISA showed that the circulating and abdominal fluid levels of DPP4 (Fig. 7D and F) were significantly higher in LPS than those in SC and LPS + dulaglutide, and were higher in LPS + dulaglutide than in SC, whereas the levels of GLP-1 (Fig. 7C and E) in circulation and in the abdominal fluid exhibited an opposite pattern to DPP4 among the groups. Additionally, blood samples from the jugular vein showed that the concentration of FITC-dextran at 10, 20 and 30 min, an indicator of peritoneal permeability, exhibited a pattern similar to that of DPP4 (Fig. 7G-I). These findings confirm that endotoxin (derived from LPS) significantly compromised the integrity of the peritoneum.

Furthermore, flow cytometric analysis demonstrated that the circulatory and abdominal-fluid levels of CD11b/c⁺ (Figs. 7J, 7M, S9A and S9D), MPO⁺ (Figs. 7K, 7N, S9B and S9E) and Ly6G⁺ cells (Figs. 7L, 7O, S9C and S9F), all indicators of inflammation, displayed a pattern identical to DPP4 among the groups.

As anticipated, the hyperplasia and thickness of the mesothelial layer of the peritoneum (Fig. 8A-E) were significantly greater in LPS group compared with those in SC group, and these changes were significantly reversed in LPS + dulaglutide group. Additionally, Masson's trichrome staining (Fig. 8F-I) revealed that the fibrotic area in the mesothelial layer of the peritoneum was significantly larger in LPS group than in SC group and LPS + dulaglutide, and also significantly larger in LPS + dulaglutide compared with in SC. These finding suggested that endotoxin, frequently released in the ESRD setting, may consistently cause damage to the mesothelial layer, potentially leading to PD failure.