Human thyroid cancer cell lines TPC-1 and 8305C were purchased from Cell Resource Center, Shanghai Institute for Biological Sciences, Chinese Academy of Sciences (https://www.cellbank.org.cn/index.php). The normal human thyroid epithelial cell line Nthy-ori 3–1 was used as a non-malignant control, and was purchased from Procell Life Science & Technology Co., Ltd. TPC-1 is a papillary thyroid carcinoma cell line and represents differentiated thyroid cancer, whereas 8305C is an anaplastic thyroid carcinoma cell line and represents a highly aggressive and poorly differentiated thyroid cancer subtype. These two cell lines were selected to evaluate the antitumor effect of polyphyllin II in thyroid cancer models with different histological origins and malignant potential.

TPC-1, 8305C, and Nthy-ori 3-1 cells were cultured in Dulbecco's Modified Eagle Medium (DMEM; Wisent Biotechnology; cat. no. 319-005-CL) supplemented with 10% fetal bovine serum (Wisent Biotechnology; cat. no. 086-150), 100 U/ml penicillin (Wisent Biotechnology; cat. no. 450-201-EL), and 100 µg/ml streptomycin (Wisent Biotechnology; cat. no. 450-201-EL). Cells were maintained in a humidified incubator at 37°C with 5% CO₂.

Polyphyllin II was dissolved in dimethyl sulfoxide (DMSO) to prepare a stock solution and diluted to the desired concentrations with complete culture medium immediately before use. Initially, it was determined whether there was cytotoxicity based on the half-maximal inhibitory concentration (IC₅₀). Finally, 5 µg/ml was selected for the subsequent cell experiments.

Lentiviral vectors used for HRH1 knockdown and overexpression were constructed by GeneChem Co., Ltd. For HRH1 silencing, a short interfering (sh)RNA sequence targeting human HRH1 was designed as follows: sh-HRH1, 5′-GCTCTGGTTCTATGCCAAGAT-3′. A non-targeting shRNA sequence, 5′-TTCTCCGAACGTGTCACGT-3′, was used as the negative control (sh-NC). For HRH1 overexpression, the full-length human HRH1 coding sequence was cloned into a lentiviral overexpression vector to generate overexpression (OE)-HRH1, while the corresponding empty vector was used as the NC.

Lentiviral particles were produced using a third-generation lentiviral packaging system. Briefly, 293T cells were obtained from the Cell Resource Center, Shanghai Institute for Biological Sciences, Chinese Academy of Sciences and cultured in DMEM supplemented with 10% FBS (Procell Life Science & Technology Co., Ltd.; cat. no. PM150210B). When the cells reached 70–80% confluence, they were co-transfected with the lentiviral expression plasmid, packaging plasmids and envelope plasmid at a mass ratio of 4:3:2:1 using Lipofectamine^® 3000 reagent (Invitrogen; Thermo Fisher Scientific, Inc.) according to the manufacturer's instructions. The total amount of plasmid DNA used for each 10-cm dish was 20 µg. The culture supernatant containing lentiviral particles was collected at 48 and 72 h after transfection, centrifuged at 1,000 × g for 10 min at 4°C to remove cell debris and filtered through a 0.45-µm filter. TPC-1 and 8305C cells were transduced with the indicated lentiviral particles in the presence of 5 µg/ml polybrene (Shanghai Yeasen Biotechnology Co., Ltd.; cat. no. 40804ES76). The multiplicity of infection was 20 for TPC-1 cells and 30 for 8305C cells. Following 48–72 h of transduction, stable cells were selected using 2 µg/ml puromycin (Shanghai Yeasen Biotechnology Co., Ltd.; cat. no. 727136ES01) for 7 days and maintained in medium containing 1 µg/ml puromycin. The efficiency of HRH1 knockdown or overexpression was verified by reverse transcription-quantitative PCR and western blotting before subsequent experiments.

The GSE197443 dataset was obtained from the Gene Expression Omnibus database (https://www.ncbi.nlm.nih.gov/gds) and differentially expressed gene analysis was performed using the GEO2R online tool (https://www.ncbi.nlm.nih.gov/geo/geo2r/). The resulting data were imported into TBtools II software (version 2.096; http://github.com/CJ-Chen/TBtools) to create volcano plots. The simplified molecular input line notation information of polyphyllin II was obtained from the PubChem database (https://pubchem.ncbi.nlm.nih.gov/) and imported into the SwissTarget database (http://www.swisstargetprediction.ch/) to predict its potential target genes. The intersection of upregulated differentially expressed genes and polyphyllin II target genes was visualized using the Venn diagram plugin of TBtools II software. The RNA sequencing data of The Cancer Genome Atlas (TCGA)-thyroid cancer (THCA) project were downloaded and processed from the TCGA database (https://portal.gdc.cancer.gov). Gene expression profiles were analyzed using the stats package (version 4.3.2, http://www.r-project.org/) and car package(version 3.1–2, http://cran.r-project.org/package=car), while single-gene differential association analysis was conducted using the DESeq2 package(version 1.52.0, http://bioconductor.org/packages/DESeq2/). Enrichment analysis was employed to identify Gene Ontology (GO) and Kyoto Encyclopedia of Genes and Genomes (KEGG) functional annotations. GO analysis and KEGG pathway analysis were performed using the clusterProfiler package (version 4.20.0, http://bioconductor.org/packages/clusterProfiler/) with a significance threshold of q<0.05.

TPC-1 and 8305C cells were seeded into 96-well plates at a density of 5×10⁴ cells/well. Following cell adherence, cells were treated with 0, 1, 5, 10 and 20 µg/ml polyphyllin II or vehicle control for 24 h at 37°C. Following incubation, 10 µl CCK-8 reagent (Beyotime Biotechnology; cat. no. C0037) was added to each well and incubated for 2 h at 37°C. The absorbance was measured at 450 nm using a microplate reader to assess proliferation activity.

TPC-1 and 8305C cells were seeded into six-well plates and treated with 5 µg/ml polyphyllin II or vehicle control for 24 h at 37°C. After treatment, cells were harvested, washed with cold phosphate-buffered saline (PBS) and resuspended in binding buffer. The cells were then stained with Annexin V- fluorescein isothiocyanate (FITC) and propidium iodide according to the manufacturer's instructions. After incubation for 15 min at room temperature in the dark, apoptotic cells were detected using a flow cytometer (LongCyte; Beijing Challen Biotechnology Co., Ltd.). Flow cytometry data were acquired and analyzed using ModelFlower software (version 2.0, Beijing Challen Biotechnology Co., Ltd.). The apoptosis rate was calculated as the percentage of early and late apoptotic cells. Each experiment was independently repeated at least three times.

TPC-1 and 8305C cells were seeded into six-well plates and treated with 5 µg/ml polyphyllin II or vehicle control for 24 h at 37°C. After treatment, cells were harvested, washed twice with cold PBS, and fixed with 70% ethanol at 4°C overnight. The fixed cells were then washed with PBS and incubated with propidium iodide/RNase staining solution for 30 min at room temperature in the dark according to the manufacturer's instructions. After incubation for 30 min at room temperature in the dark, cell cycle distribution was analyzed using a flow cytometer (LongCyte; Beijing Challen Biotechnology Co., Ltd.). Flow cytometry data were acquired and analyzed using ModelFlower software (version 2.0, Beijing Challen Biotechnology Co., Ltd.). The percentages of cells in the G₀/G₁, S, and G₂/M phases were calculated. Each experiment was independently repeated at least three times.

The upper chambers of Transwell inserts (MilliporeSigma; cat. no. PI8P01250) were precoated with Matrigel matrix (MilliporeSigma; cat. no. CLS356237) and air-dried at 37°C for 2 h to allow gel formation. TPC-1 and 8305C cells were pretreated with 5 µg/ml polyphyllin II or vehicle control for 24 h at 37°C before being seeded into the upper chambers. Cells suspended in serum-free medium were added to the upper chambers at a density of 5×10⁵ cells/well, while complete medium containing 10% fetal bovine serum (Wisent Biotechnology; cat. no. 086-150) was added to the lower chambers as a chemoattractant. Following incubation for 24 h at 37°C, the cells that invaded through the membrane were fixed with 2.5% paraformaldehyde (Coolaber; cat. no. SL1770) for 20 min at room temperature and stained with 0.1% crystal violet (Beyotime Biotechnology; cat. no. C0121) for 20 min at room temperature. The number of invaded cells was imaged and quantified under a microscope.

The cells were seeded into six-well plates at a density of 2×10⁵ cells/well and grown to 100% confluence. A sterile 200 µl pipette tip was used to scratch straight lines on the monolayer surface. Detached cells were washed away with PBS and the remaining cells were incubated with serum-free medium containing 5 µg/ml polyphyllin II according to group allocation. Images of the wounded area were captured at 0, 12 and 24 h using an inverted light microscope (DM2700M; Leica Microsystems GmbH). Cell migration was quantified by measuring the wound area at each time point using ImageJ software (version 1.53t, National Institutes of Health). The wound closure rate was calculated as follows: wound closure rate (%)=[(wound area at 0 h - wound area at indicated time point)/wound area at 0 h] ×100. Each experiment was independently repeated at least three times.

TPC-1 and 8305C cells were seeded into six-well plates at a density of 2×10⁵ cells/well. After the indicated treatments, total RNA was extracted using RNAiso Plus reagent (Takara Bio, Inc.; cat. no. 9108) according to the manufacturer's protocol, and RNA concentration and purity were assessed via spectrophotometry. cDNA synthesis was performed using the designated reverse transcription kit (Takara Bio, Inc.; cat. no. RR047) according to the manufacturer's protocol. GAPDH was used as the internal control. The PCR cycling conditions were: Initial denaturation at 95°C for 30 sec, followed by 40 cycles of denaturation at 95°C for 5 sec and annealing/extension at 60°C for 30 sec. qPCR was conducted using TB Green Premix Ex Taq II (Takara Bio, Inc.; cat. no. RR820A) on a real-time PCR detection system. The relative gene expression levels were calculated using the 2^−ΔΔCq method (13). Each experiment was independently repeated at least three times.

The primer sequences were: HRH1-F: GCAGGGACTATGTAGCCGTC; HRH1-R: GCCTGTGTTAGACCCACTCC; GAPDH-F: CAGGAGGCATTGCTGATGAT; GAPDH-R: GAAGGCTGGGGCTCATTT.

Total cellular protein was extracted using RIPA lysis buffer (Beijing Solarbio Science & Technology Co., Ltd.; cat. no. R0010) containing protease and phosphatase inhibitors. Protein concentration was determined using a BCA protein assay kit (Beyotime Biotechnology; cat. no. P0010) according to the manufacture's protocol. The protein samples (30 µg/lane) were separated by 10% SDS-PAGE (Beijing Solarbio Science & Technology Co., Ltd.; cat. no. P1040), transferred to polyvinylidene difluoride membranes and blocked with 5% non-fat milk in Tris-buffered saline containing 0.1% Tween-20 (HuShi; cat. no. 30189328) for 1 h at room temperature. Subsequently, the membranes were incubated overnight at 4°C with primary antibodies against HRH1 (Beyotime Biotechnology; cat. no. P70174), Wnt7A (Beyotime Biotechnology; cat. no. AF8361), MMP7 (Beyotime Biotechnology; cat. no. AF7485), β-catenin (Beyotime Biotechnology; cat. no. AC106) and GAPDH (Beyotime Biotechnology; cat. no. AF0006). After washing with Tris-buffered saline containing 0.1% Tween-20, the membranes were incubated with HRP-conjugated goat anti-rabbit IgG secondary antibody (1:5,000; Beyotime Biotechnology; cat. no. A0208) or HRP-conjugated goat anti-mouse IgG secondary antibody (1:5,000; Beyotime Biotechnology; cat. no. A0216) for 1 h at room temperature. Protein bands were visualized using an enhanced chemiluminescence reagent (Beyotime Biotechnology) and quantified using ImageJ software (version 1.53t; National Institutes of Health). GAPDH was used as the loading control. Each experiment was independently repeated at least three times.

Molecular docking was performed to evaluate the potential interaction between polyphyllin II and HRH1. The chemical structure of polyphyllin II was obtained from the PubChem database, and the protein structure of HRH1 was obtained from the Protein Data Bank (https://www.rcsb.org/) or a predicted structural database. The ligand and receptor structures were prepared by removing water molecules, adding hydrogen atoms, and assigning charges. Docking analysis was then performed using AutoDock Vina (version 1.2.5, http://vina.scripps.edu/). The docking pose with the lowest binding energy was selected for further visualization, and the interaction between polyphyllin II and HRH1 was analyzed using PyMOL (version 2.5.4).

To verify whether HRH1 is a potential target of the polyphyllin II, cell lysates were incubated with polyphyllin II or vehicle control, followed by pronase digestion. HRH1 protein levels were then detected by WB. Increased resistance of HRH1 to protease digestion indicated the interaction between polyphyllin II and HRH1.

For the in vivo xenograft experiments, 8305C cells were selected as anaplastic thyroid carcinoma is more aggressive and clinically challenging and 8305C cells are suitable for evaluating tumor growth inhibition in a highly malignant thyroid cancer model. A total of 30 male BALB/c nude mice aged 4–6 weeks and weighing 18–22 g were purchased from Charles River Laboratories Co., Ltd. The mice were housed under specific pathogen-free conditions at 22±2°C with 50–60% relative humidity and a 12-h light/dark cycle, with free access to food and water. Following 1 week of acclimatization, 1×10⁶ tumor cells were subcutaneous injected into the right dorsal flank of each mouse. Once tumor volumes approximately 100 mm³, the mice were randomly assigned to five groups (n=6 per group), including TC, TC + polyphyllin II, NC, HRH1 knockdown (sh-HRH1) and HRH1 overexpression plus polyphyllin II treatment (OE HRH1 + polyphyllin II) groups. The control mice received intraperitoneal injections of vehicle solution (normal saline or DMSO diluent), while the treated mice were administered polyphyllin II (20 mg/kg/d) or subjected to lentiviral-mediated HRH1 modulation for 2–4 weeks. Tumor dimensions were measured every 2 days using vernier calipers and tumor volume was calculated as (length × width²)/2 to generate growth curves.

Mice were monitored daily for general health status, behavior, food and water intake, body weight, tumor growth and tumor-related discomfort. Tumor dimensions were measured every 2 days using vernier calipers, and tumor volume was calculated as (length × width²)/2. Humane endpoints were predefined as tumor volume >1,500 mm³, tumor ulceration, necrosis or bleeding, impaired mobility, inability to access food or water, severe lethargy, persistent hunching, respiratory distress, or body weight loss >20% of baseline body weight. Mice that reached any humane endpoint were immediately sacrificed. At the end of the experiment, mice were deeply anesthetized with sodium pentobarbital at 50 mg/kg by intraperitoneal injection. Adequate depth of anesthesia was confirmed by the absence of pedal withdrawal and corneal reflexes. Cervical dislocation was then performed under deep anesthesia by trained personnel. Mortality was confirmed by the absence of respiration, heartbeat and reflex responses before tumor tissues were collected. All animal procedures were conducted in accordance with the ARRIVE guidelines and the AVMA Guidelines for the Euthanasia of Animals: 2020 Edition (https://www.avma.org/resources-tools/avma-policies/avma-guidelines-euthanasia-animals) and were approved by the Ethics Committee of The Fifth Affiliated Hospital of Kunming Medical University (approval no. kmmu20240805).

During the treatment period, mice were monitored daily for general health status, behavior, food and water intake, activity, body weight, tumor growth and tumor-related discomfort. No obvious treatment-related mortality or severe adverse effects were observed during the experimental period. Body weight was recorded regularly as a general indicator of systemic tolerability. The maximum tumor volume measured in this study was 880 mm³, and the maximum tumor diameter did not exceed 12 mm.

Tumor tissues were fixed in 4% paraformaldehyde (Sinopharm Chemical Reagent Co., Ltd.; cat. no. 30525-89-4) for 24 h at room temperature. The tissues were dehydrated through a graded ethanol series (Sinoparm Chemical Reagent Co., Ltd.; cat. no. 100092683), including 70, 80, 90, 95 and 100% ethanol, cleared in xylene and embedded in paraffin (Sinoparm Chemical Reagent Co., Ltd.; cat. no. 1330-20-7). Paraffin-embedded tumor tissues were cut into 4-µm-thick sections. After deparaffinization and rehydration, the sections were stained with hematoxylin (Baso Diagnostics; cat. no. BA4097) for 5 min at room temperature and eosin (Baso Diagnostics; cat. no. BA4099) for 2 min at room temperature. The sections were then dehydrated, cleared, mounted with neutral resin and observed under a light microscope.

Immunohistochemical staining was performed on 4-µm-thick paraffin-embedded tumor tissue sections. After deparaffinization in xylene and rehydration through a graded ethanol series, antigen retrieval was performed by heating the sections in citrate antigen retrieval buffer at 95°C for 15 min. Endogenous peroxidase activity was blocked with 3% hydrogen peroxide for 10 min at room temperature. The sections were then blocked with 5% goat serum for 30 min at room temperature and incubated with anti-Ki67 antibody (Abcam; cat. no. ab16667; 1:300) overnight at 4°C. After washing with phosphate-buffered saline, the sections were incubated with HRP-conjugated goat anti-rabbit IgG secondary antibody (Dako; Agilent Technologies, Inc.; cat. no. K4003, 1:500) for 30 min at room temperature. Immunoreactivity was visualized using a DAB chromogen detection kit, and the sections were counterstained with hematoxylin for 2 min at room temperature. Finally, the sections were dehydrated, cleared, mounted and observed under a light microscope. Images were acquired at ×20 and ×40 magnification.

All experiments were independently repeated at least three times. Data are presented as the mean ± standard deviation. Statistical analyses were performed using GraphPad Prism software version 9.0 (Dotmatics). The normality of data distribution was assessed using the Shapiro-Wilk test before applying parametric tests. For comparisons between two groups, Student's t-test was used for normally distributed data. For comparisons among multiple groups, one-way ANOVA followed by Tukey's post hoc test was performed. Spearman correlation analysis was used to evaluate the correlation between HRH1 expression and Wnt/β-catenin signaling pathway-related genes in The Cancer Genome Atlas-thyroid carcinoma dataset. Effect sizes were considered where appropriate to support the interpretation of biologically meaningful differences. P<0.05 was considered to indicate a statistically significant difference.

CCK-8 assays demonstrated that polyphyllin II markedly reduced the viability of thyroid cancer cells in a dose-dependent manner (Fig. 1A). Based on the IC₅₀ value, it was ultimately determined that 5 µg/ml was the final experimental concentration. Flow cytometry analysis further revealed a significant increase in apoptotic cell populations following polyphyllin II treatment (Fig. 1B). Cell cycle analysis showed that polyphyllin II markedly increased the G₀/G₁-phase population in both 8305C and TPC-1 cells, while reducing the G₂/M-phase population. These results indicate that polyphyllin II induces G₀/G₁-phase cell cycle arrest, which may contribute to its anti-proliferative effect in thyroid cancer cells (Fig. 1C). Transwell invasion assays indicated that polyphyllin II attenuated the invasive capacity of 8305C and TPC-1 cells, whereas wound healing assays indicated impaired migratory ability following treatment (Fig. 1D and E). These findings indicate that polyphyllin II effectively restrains thyroid cancer progression by inhibiting proliferation and metastatic behavior.

Differential gene expression analysis revealed significant transcriptomic alterations in thyroid cancer, with 910 genes upregulated and 827 downregulated compared with non-tumor tissues (Fig. 2A). Target prediction using SwissTarget and intersection analysis identified 13 upregulated genes potentially associated with polyphyllin II (Fig. 2B and C). TCGA and GEO dataset validation confirmed that the expression levels of HRH1, LGALS1, ADORA1 and ECE1 were significantly elevated in thyroid cancer (Fig. 2D and E). Among these genes, HRH1 has been reported as an oncogenic mediator in multiple cancer types through regulation of cell survival, angiogenesis, immune modulation and invasion (14,15), suggesting its potential role in thyroid cancer progression.

RT-qPCR analysis confirmed that the expression levels of HRH1, LGALS1, ADORA1 and ECE1 were markedly upregulated in thyroid cancer cells (Fig. 3A). Western blotting further validated elevated protein levels of these targets, with HRH1 indicating notably high expression in TPC-1 and 8305C cells (Fig. 3B). Given that HRH1 signaling mediates histamine-induced tumor proliferation and immune escape across multiple malignancies, HRH1 was selected as the primary candidate for further investigation.

To determine whether HRH1 is a direct target of polyphyllin II, molecular docking and DARTS assays were performed. Molecular docking showed that polyphyllin II could fit into the predicted binding pocket of HRH1, suggesting a potential interaction between polyphyllin II and HRH1 (Fig. 4A). Consistently, DARTS assay showed that polyphyllin II increased the resistance of HRH1 protein to pronase digestion, further supporting the direct interaction between polyphyllin II and HRH1 (Fig. 4B).

The present study next modulated HRH1 expression in thyroid cancer cells. RT-qPCR and western blot results confirmed that sh-HRH1 significantly reduced HRH1 expression, whereas OE-HRH1 markedly increased HRH1 expression (Fig. 4C-F). These results indicated that HRH1 can be directly targeted by polyphyllin II and that the HRH1 knockdown and overexpression models were successfully established for subsequent functional experiments.

To determine the functional role of HRH1 in thyroid cancer cells, HRH1 was silenced using sh-HRH1. CCK-8 assays showed that HRH1 knockdown significantly reduced the proliferation of both 8305C and TPC-1 cells compared with the control and sh-NC groups (Fig. 5A and B). Flow cytometry further showed that sh-HRH1 increased the apoptosis rate in both cell lines (Fig. 5C). In addition, Transwell assays demonstrated that HRH1 knockdown markedly decreased the invasive ability of 8305C and TPC-1 cells (Fig. 5D). Wound-healing assays also showed that sh-HRH1 delayed wound closure, indicating impaired migratory capacity after HRH1 silencing (Fig. 5E). These results suggest that HRH1 promotes malignant phenotypes in thyroid cancer cells.

Overexpression of HRH1 counteracted apoptosis and enhanced invasive and migratory abilities in TPC-1 and 8305C cells, whereas polyphyllin II administration reversed these effects (Fig. 6A-E). These results suggest that polyphyllin II inhibits thyroid cancer malignancy in part by attenuating HRH1 signaling. Given that HRH1 acts as a downstream regulator of histamine signaling and oncogenic activity, these findings provide a mechanistic basis for using polyphyllin II as a potential HRH1-targeted therapeutic strategy.

Previous evidence suggests that histamine receptor H1-related signaling may activate canonical β-catenin signaling, while Wnt/β-catenin activation is closely associated with thyroid cancer progression (16–18). Consistently, TCGA-THCA single-gene correlation analysis showed that HRH1 was positively correlated with several Wnt/β-catenin-related genes, including MMP7, WNT7A, CCND1, TCF7, CTNNB1 and MYC (Fig. S1). These findings provided a rationale for subsequent experimental validation. Knockdown of HRH1 expression significantly reduced the expression levels of the β-catenin pathway-related genes (MMP7, Wnt7A and β-catenin) and decreased β-catenin nuclear translocation, whereas polyphyllin II treatment further suppressed pathway activation (Fig. 7A and B). Conversely, HRH1 overexpression enhanced β-catenin signaling, while polyphyllin II blocked this activation, indicating an HRH1-dependent regulatory mechanism. Therefore, polyphyllin II may exert antitumor effects in thyroid cancer by suppressing HRH1-mediated β-catenin activation.

To validate the in vivo findings, xenograft models were established using 8305C cells in nude mice. The growth transplanted 8305C xenograft tumors in mice was accelerated significantly. During the in vivo treatment period, no obvious treatment-related toxicity was observed. Mice in the polyphyllin II-treated group showed no marked abnormalities in general behavior, activity, food intake or water intake. Body weight remained relatively stable throughout the experiment, suggesting that polyphyllin II was generally tolerated under the present treatment conditions. The mice that were treated with polyphyllin II demonstrated a significant reduction in tumor size, indicating that polyphyllin II exhibited an inhibitory effect on tumors (Fig. 8A-D). The tumor tissues were stained using IHC analysis for H&E and Ki67. The results indicated that polyphyllin II could alleviate the deterioration of the tumor tissues and reduce cancer cell proliferation (Fig. 8E and F). WB results indicated that the expression levels of the proteins of the HRH1 signaling pathway were reduced following the use of polyphyllin II (Fig. 8G).

To further confirm the effect of polyphyllin II on the HRH1 signaling pathway, 8305C cells were divided into three groups; NC, lentiviral sh-HRH1 and lentiviral OE-HRH1 combined with polyphyllin II treatment. Compared with NC, following knockdown of HRH1 expression, the tumor size decreased. Following IHC staining with H&E and Ki67, the severity of tumor tissue deterioration decreased and the proliferation of the cells was reduced (Fig. 9A-D). Following treatment of the tumor-bearing mice expressing HRH1 with polyphyllin II, the volumes of the tumors were reduced. The tissue staining results indicated that the severity of tumor tissue deterioration and cellular proliferation were reduced (Fig. 9E and F). WB results also demonstrated that polyphyllin II inhibited tumor growth by suppressing the HRH1 signaling pathway (Fig. 9G).