Abstract
Annexin A10 (ANXA10) belongs to a family of membrane-bound calcium-dependent phospholipid-binding proteins, but its precise function remains unclear. Further research is required to understand its role in sessile serrated lesions (SSL) and colorectal cancer (CRC). We conducted transcriptome sequencing on pairs of SSL and corresponding normal control (NC) samples. Bioinformatic methods were utilized to assess ANXA10 expression in CRC. We knocked down and overexpressed ANXA10 in CRC cells to examine its effects on cell malignant ability. The effect of ANXA10 on lung metastasis of xenograft tumor cells in nude mice was also assessed. Furthermore, we used quantitative polymerase chain reaction, western blotting, and flow cytometry for reactive oxygen species (ROS), lipid ROS, and intracellular Fe2+ to measure ferroptosis. Immunoblotting and Immunofluorescence staining were used to detect autophagy. We found that ANXA10 was significantly overexpressed in SSL compared to NC. ANXA10 was also highly expressed in BRAF mutant CRCs and was associated with poor prognosis. ANXA10 knockdown reduced the survival, proliferation, and migration ability of CRC cells. Knockdown of ANXA10 inhibited lung metastasis of CRC cells in mice. ANXA10 knockdown increased transferrin receptor (TFRC) protein levels and led to downregulation of GSH/GSSG, increased Fe2+, MDA concentration, and ROS and lipid ROS in cells. Knockdown of ANXA10 inhibited TFRC degradation and was accompanied by an accumulation of autophagic flux and an increase in SQSTM1. Finally, Fer-1 rescued the migration and viability of ANXA10 knockdown cell lines. In brief, the knockdown of ANXA10 induces cellular ferroptosis by inhibiting autophagy-mediated TFRC degradation, thereby inhibiting CRC progression. This study reveals the mechanism of ANXA10 in ferroptosis, suggesting that it may serve as a potential therapeutic target for CRC of the serrated pathway.
Similar content being viewed by others
Introduction
Colorectal cancer (CRC) is the third most commonly diagnosed cancer worldwide and the second leading cause of cancer death for both sexes [1]. In addition to the traditional adenoma-carcinoma sequence, the serrated pathway is the other major pathway leading to CRC. This pathway is characterized by the presence of a serrated lesion (SL) as a precancerous lesion [2]. However, previously, colorectal SL was misinterpreted as a harmless lesion and classified as hyperplastic polyps (HPs) [3]. In the last decade, intensive research has revealed that SL is one of the leading causes of “interstitial cancer”. Approximately 25% of sporadic CRCs develop through SL [4]. According to the latest WHO classification of gastrointestinal tumors (5th edition) published in 2019, colorectal SL is classified into four categories: HPs, sessile serrated lesions (SSL), and sessile serrated lesions with dysplasia (SSLD), traditional serrated adenomas (TSAs) and unclassified SL [5].
Of these, SSL is thought to have malignant potential, progressing rapidly to CRC in a short period. Two case reports have reported rapid progression to invasive tumors at 8 and 13 months, respectively [6, 7]. SSL is easily overlooked during colonoscopy as they present as pale, ill-defined flat lesions with a mucous surface often adhering in a “cloudy” appearance. This feature allows SSL to escape detection and further contributes to their progression [8]. At the molecular level, the BRAFV600E mutation and the CpG island methylator phenotype-high (CIMP-H) are the two main features of SSL and the sessile serrated carcinoma pathway [9, 10]. However, the mechanisms of SSL and serrated carcinoma pathway development remain poorly understood.
Annexin A10 (ANXA10, A10) is a member of the calcium-dependent phospholipid-binding protein family, whose function has not yet been determined [11]. Several studies have found that ANXA10 is specifically highly expressed in colon SSL and MSI-H CRC [12,13,14,15,16], but its mechanism of action has not been investigated in depth. In other different cancers, ANXA10 has been associated with distinct roles, with high expression in some cancers, such as melanoma [17], extrahepatic cholangiocarcinoma [18], esophageal epithelial squamous cell carcinoma [19], and oral cancer [20] being associated with worse prognosis, whereas it acts as a protective factor in other cancers, such as liver cancer [21], prostate cancer [22], and bladder cancer [23]. Therefore, the role of ANXA10 in SSL and CRC needs to be further investigated.
In this study, ANXA10 was identified as a molecule differentially expressed in SSL and the serrated pathway by transcriptome sequencing. The specific molecular mechanisms of ANXA10 were investigated to seek out potential targets for intervention, paving the way for precise prevention and treatment of CRC.
Methods and materials
Patient samples
This study utilized 12 pairs of sessile serrated colorectal lesions, matched normal control specimens, and colon cancer specimens obtained from Renji Hospital, Shanghai Jiao Tong University School of Medicine. The pathological diagnosis of these lesions was conducted in accordance with the latest edition of the WHO diagnostic criteria for serrated lesions in 2019 [5]. All clinical specimens underwent postoperative pathological confirmation. Our study was approved by the Ethics Committee of Renji Hospital, Shanghai Jiao Tong University School of Medicine (KY2021-004). All patients provided informed consent.
Antibodies and chemicals
Antibodies against ANXA10 (ab213656), β-Actin (ab8227), LC3B (ab192890), and SQSTM1 (ab109012) were purchased from Abcam (USA). Rabbit anti-β-Tubulin (#2128) antibody was purchased from Cell Signaling Technology. Rabbit anti-TFRC (10084-2-AP) was purchased from Proteintech, and mouse anti-Flag (DYKDDDDK-Tag) was purchased from Abmart. LAMP1 antibody (sc-20011) was purchased from Santa Cruz (CA, USA). Alexa Fluor 488 (A-21202) and Alexa Fluor 594 (A-21207) conjugated secondary antibodies were purchased from Invitrogen (CA, USA). Ferrostatin-1 (HY-100579), Deferoxamine mesylate (HY-B0988), Rapamycin (HY-10219), and Chloroquine (HY-17589A) were purchased from MedChemExpress. Cycloheximide (S7418) was purchased from Selleck, and DMSO (D2650) and N-acetyl-L-cysteine (A9165) were purchased from Sigma-Aldrich. Hydrogen peroxide solution (88597) was purchased from Millipore.
Cell death, viability, and proliferation assays
Cell death was assessed using either the Annexin V-FITC Apoptosis Detection Kit I (BD Biosciences, USA) or the Annexin V-PE/7-AAD Apoptosis Detection Kit (Vazyme, Nanjing, China) in accordance with the manufacturer’s instructions. The proportion of cell death was subsequently measured by flow cytometry. Cell viability was determined using the Cell Counting Kit-8 (CCK-8) (Dojindo, Japan) as per the manufacturer’s recommendation. To measure cell proliferation, the CCK-8 (Dojindo, Japan) was used following the manufacturer’s instructions.
Cell culture, transfection, and generating stable cell lines
The human colorectal cancer cell lines used in this study (HT29, HCT116, SW480, and RKO) were obtained from American Type Culture Collection (ATCC). Of these, HT29 and RKO cells carry the BRAF V600E mutation, while HCT116 and SW480 cells have the wild-type BRAF gene. HT29 and HCT116 cells were cultured in McCoy'5a medium, while SW480 and RKO cells were cultured in RPMI 1640 medium (both from Gibco, USA). In addition, 10% fetal bovine serum and 1% penicillin–streptomycin (both from Gibco, USA) were added to the respective media. All cell lines were incubated at 37 °C in a 5% CO2 atmosphere.
The day before transfection, well-grown cells were seeded onto plates following the manufacturer’s instructions. Once the cells reached 60–80% confluence, small-interfering RNAs (siRNAs) and the plasmid were transfected using DharmaFECT 1 siRNA transfection reagent (Horizon Discovery Ltd., USA) and FuGene HD transfection reagent (Promega, Madison, WI, USA), respectively. The siRNAs were purchased from GenePharma Technology (Shanghai, China), while the plasmid and LV-ANXA10-shRNA were obtained from GeneChem (Shanghai, China). To achieve knockdown, Lentiviral-packed shRNA was used to infect HT29 cells with HiTransG P according to the manufacturer’s protocol. After 72 h, positive cells were selected using puromycin (8 μg/ml) for 2–3 generations to establish cell lines that were stably infected with shRNA. The plasmid and shRNA constructs used were GV492 and GV493 and the sequences of siRNAs and shRNA are listed in Table S1.
In vivo mouse xenograft models
For the in vivo xenograft mouse model, 5-week-old BALB/c male nude mice were purchased from GemPharmatech Co. Ltd. (Nanjing, China) and kept in specific pathogen-free conditions at 25 °C with suitable humidity and a light/dark cycle. To create a single-cell suspension, 1 × 106 shNC or shANXA10 HT29 cells were dissolved in 200 μL PBS and mixed. The mice were randomly divided into two groups (n = 5 per group) and injected with the single-cell suspension through the tail vein. After eight weeks, the mice were sacrificed, and their lung tissues were extracted, observed, and photographed. The tissues were fixed in formalin for 24 h, embedded in paraffin, and stained with H&E. All study procedures were approved by the Institutional Animal Care and Use Committee of Renji Hospital, School of Medicine, Shanghai Jiaotong University.
Immunohistochemistry (IHC)
SSL, CRC, and normal colon tissues were obtained from Renji Hospital, Shanghai Jiao Tong University School of Medicine, and all samples were formalin-fixed and embedded in paraffin tissue blocks. The tissue blocks were sectioned into 4 μm slices. After deparaffinization and antigen retrieval, the sections were incubated with 3% hydrogen peroxide solution for 20 min to quench endogenous peroxidase activity and with goat serum for 30 min to block nonspecific binding. Next, the sections were incubated overnight at 4 °C with an anti-human ANXA10 antibody (1:200) and for 30 min at room temperature with a horseradish peroxidase-conjugated secondary antibody. The sections were then visualized with 3,3-diaminobenzidine substrate and counterstained with hematoxylin before observation under a light microscope.
Immunofluorescence staining
HT29 cells were seeded at a density of 2 × 104 cells/well into a Nunc™ Lab-Tek™ II 8-well Chambered Slide (Thermo Fisher Scientific, Rochester, NY, USA) and transfected with siRNA after 24 h. Cells were further cultured for 48 h and then fixed with 4% paraformaldehyde for 30 min. Cells were washed three times in PBS, permeabilized by 0.3% Triton X-100 for 30 min, and blocked using 1% BSA in PBS for 30 min. Cells were then incubated with primary antibodies against TFRC (1:100) and LAMP1 (1:100) overnight at 4 °C. The slide was incubated with Alexa Fluor 488- and 594-conjugated secondary antibodies for 1 h at room temperature, and followed by staining with DAPI (Southern Biotech, Birmingham, AL). Fluorescence images were photographed with FV3000 laser confocal microscope (Olympus, Japan).
Transcriptome sequencing (RNA-seq) analysis
Total RNAs were extracted from SSL, paired normal tissues, HT29-shANXA10, and HT29-shNC cells using Trizol (Invitrogen, Carlsbad, CA, USA) according to the protocol. The RNAs were subsequently qualified and quantified using NanoDrop 2000 (Thermo Fisher Scientific, MA, USA). Purified mRNA was randomly fragmented into small fragments using Oligo(dT)-attached magnetic beads at the appropriate temperature and subjected to PCR reactions to synthesize first-strand cDNA and second-strand cDNA. The reaction products were then purified using magnetic beads, followed by the addition of A-Tailing Mix and RNA Index Adapters to repair the ends and subsequent PCR amplification. The final libraries were obtained by purifying the products using Ampure XP magnetic beads, which were then assessed for quality and quantity using an Agilent 2100 bioanalyzer before undergoing DSN treatment. The DSN-treated libraries were evaluated for quality in two ways: (i) by checking the distribution of fragment sizes using the Agilent 2100 bioanalyzer and (ii) by quantifying the libraries using qPCR. Single-end sequencing was performed on the Illumina Novaseq 6000 platform (Tsingke, Beijing, China).
To examine the coherence of samples within groups and the differences in variability between groups in RNA-seq, we employed principal component analysis (PCA) to analyze all samples. The analysis and visualization of results were carried out using the “FactoMineR” and “factorextra” R packages. For the identification of differentially expressed genes (DEG), we conducted an enrichment analysis of the Kyoto Encyclopedia of Genes and Genomes (KEGG) signaling pathway using the “clusterProfiler” R package. The enrichment results were then presented graphically using the “enrichplot” R package.
Single-cell transcriptome sequencing analysis
The different types of intestinal epithelial cells were clustered and grouped using the R package “Seurat” (version 4.0.3). Other analysis steps were based on our previous study [24]. Ultimately, we discovered eight significant epithelial cell types in the SL, including a specific subpopulation unique to the SL, which we named Epi-SL. We then compared the expression levels of ANXA10 in the eight distinct cell subpopulations.
Quantitative real-time polymerase chain reaction (qPCR)
To extract total RNA from cells, we utilized Trizol (Invitrogen, Carlsbad, CA, USA) according to the manufacturer’s instructions. The extracted RNA was assessed for quality and quantity using NanoDrop 2000 (Thermo Fisher Scientific, MA, USA), followed by reverse transcription to cDNA using a PrimeScript RT Reagent Kit (Takara, Japan). Quantitative RT-PCR was then conducted using SYBR Premix Ex Taq (Takara, Japan) in accordance with the manufacturer’s guidelines. The expression levels of mRNAs were normalized to β-Actin. Table S2 contains the sequences of all primers used in the experiment.
Wound-healing assay and transwell assay
Wound-healing assays and transwell assays were performed to assess the migration capacity of the cells. For the wound-healing assay, cells were plated in 6-well plates at a density of 4 × 105 cells per well and transfected with plasmids the following day. Once the cells reached 90% confluence, they were vertically scratched in the plate using a sterile 200 μL gun tip. After washing twice with PBS, the cells were cultured in a serum-free medium. Microscopic images were captured at 0 h and 40 h, and the area of the scratched region was calculated relative to the 0 h time point to determine the migration rate.
For the transwell assay, 600 μL of 30% FBS medium was added to a 24-well plate, and transwell chambers (Millipore, Darmstadt, Germany) were placed on top. Next, 300 μL of cell suspension at a concentration of 1 × 106 cells/mL was added to each chamber. The cells were then incubated for 24–72 h, depending on the characteristics of the cells. After incubation, the 24-well plate was removed, and the upper chamber medium was discarded. The cells on the upper surface of the membrane were wiped off using a cotton swab, and the outer layer of the chambers was washed twice with PBS. The cells were then fixed using 600 μL of 4% paraformaldehyde for 30 min, followed by staining with 600 μL of crystalline violet staining solution for 15 min at room temperature. After washing with PBS, the cells were air-dried and observed under a microscope. Six randomly selected fields of view were photographed, and the number of cells was counted.
Measurement of lipid peroxidation and reactive oxygen species (ROS)
Cells were inoculated in plates and transfected with siRNA after 24 h. To detect levels of lipid peroxidation, the old medium was removed after 48 h of incubation, and the cells were washed once with a serum-free medium. Then, 500 μL of a 10 μM Liperfluo solution (#L248, Dojindo, Japan) diluted with serum-free medium was added to each well and incubated for 30 min at 37 °C. The cells were washed twice with serum-free medium, and then digested with trypsin. After centrifuging and resuspending with 300 μL of PBS, the fluorescence intensity of the samples was measured using flow cytometry.
To detect ROS levels, the old medium was removed after continuing incubation for 48 h, and 500 μL of a 10 μM DCFH-DA (#S0033, Beyotime Biotechnology, China) working solution prepared with serum-free medium was added to each well and incubated for 20 min at 37 °C. The cells were then washed three times with serum-free medium, and digested with trypsin, and the fluorescence intensity of the samples was determined using flow cytometry.
Immunoblotting
Whole cells were harvested and lysed in RIPA buffer supplemented with protease and phosphatase inhibitors. The lysates were then separated by SDS-PAGE and transferred onto nitrocellulose membranes. The membranes were blocked with a blocking solution, and then incubated overnight at 4 °C with primary antibodies. After washing, the membranes were incubated for 1 h at room temperature with secondary antibodies. The proteins of interest were detected by chemiluminescence using ChemiDoc Touch (Bio-Rad, California, USA). All the original western blot images were shown in supplementary information.
Glutathione (GSH) quantification and malondialdehyde (MDA) assay
Intracellular levels of all glutathione and oxidized glutathione (GSSG) were detected using the GSH/GSSG Detection Kit (#S0053, Beyotime Biotechnology, China) according to the manufacturer’s instructions. The intracellular MDA concentration was determined using a Cell Malondialdehyde Assay Kit (Colorimetric method, #A003-4-1, Nanjing Jiancheng Bioengineering Institute, China) according to the manufacturer’s recommended protocol.
Cell ferrous ion (Fe2+) level analysis
After removing the supernatant from the plate, the cells were washed three times with a serum-free medium. Subsequently, FerroOrange (1 μM, #F374, Dojindo, Japan) working solution (diluted with serum-free medium) was added and the cells were incubated for 30 min at 37 °C, as per the manufacturer’s instruction. The cells were then observed and photographed directly under a fluorescence microscope. Alternatively, cells were trypsinized, centrifuged at 1000 rpm for 5 min at 4 °C, and resuspended in 400 μL of serum-free medium. The fluorescence intensity was immediately measured using a flow cytometer.
Mass spectrometry (MS)
After protein extraction and reductive alkylation, the samples were analyzed by MS on a Thermo Fisher LTQ Qbitrap ETD Mass spectrometer. In brief, samples were placed on a Thermo Fisher Easy-nLC 1000 HPLC system equipped with a C18 column (1.8 mm, 0.15 × 1.00 mm) with solution A containing 0.1% formic acid and solution B with 100% acetonitrile. MS was performed in positive ion mode at a flow rate of 300 nL/min. FTMS was used to obtain a full scan (350–1600 m/z) at a mass resolution of 30,000, followed by MS/MS using higher-energy collisional dissociation for the 10 most intense pioneer ions at 35% collisional energy and a mass resolution of 15,000. The raw MS files were analyzed using MaxQuant (1.6.1.0). The search included dynamic modifications of methionine oxidation and deamidation and static modification of carbamidomethyl cysteine. A maximum of two missed cleavages was allowed, and the mass tolerance for precursor ions and fragment ions was set to 20 ppm and 4.5 ppm, respectively. The minimal peptide length was set to six amino acids, and a maximum of two miscleavages was allowed. The peptide and protein identifications were accepted at a false discovery rate of 0.01.
Protein degradation assay
Cells were pre-inoculated in 6-well plates with a density of 5 × 105 cells per well. The old medium was then removed, and 2 mL of the complete medium was added to each well. Cycloheximide (CHX) was added to each well at pre-set time points of 12th, 9th, 6th, and 0th hour according to the pre-set incubation time gradient of CHX (0, 3, 6, and 12 h). Therefore, we added 2 μL of 50 mg/mL of CHX to the corresponding wells at each pre-set time point, respectively, resulting in a final concentration of 50 μg/mL. After a total incubation period of 12 h, all samples were subjected to protein extraction, followed by immunoblotting analysis to determine the relative gray values of the target proteins, with β-Actin expression serving as the internal reference.
Public database analysis
The mRNA transcriptome sequencing data for Colon Adenocarcinoma (COAD) from The Cancer Genome Atlas (TCGA, http://cancergenome.nih.gov) and clinical information were obtained from the UCSC Xena database (https://xena.ucsc.edu/). The transcriptome data were converted into log2CPM (counts per million) for subsequent analysis using the “edgeR” R package. The colon cancer mRNA microarray dataset GSE39582, which includes 51 BRAF mutant CRC patients and 474 BRAF wild-type CRC patients, from the Gene Expression Omnibus (GEO) database was obtained using the “GEOquery” R package and annotated using the “clusterProfiler” R package. The survival analysis of CRC patients was done using the “survival” and “survminer” R software packages, and the cutoff value for the grouping of ANXA10 expression levels was determined using the X-tile software. The relationship between gene expression levels and clinical information was processed using the “reshape2” R package and visualized using the “ggpubr” R package.
Gene set variation analysis
GSVA analysis is used to assess the enrichment of a gene set in individual samples. This analysis was performed using the “GSVA” R package, which calculates the enrichment scores, and the “ggplot2” R package was used to visualize the data.
Statistical analysis
All statistical analyses were performed using GraphPad Prism 9.3.1 or R 4.1.2 software. For statistical analysis between two groups of samples, an independent sample t-test was used if they obeyed a normal distribution, while paired samples used a paired t-test. For three or more groups of samples, the one-way ANOVA was performed. Non-parametric tests were used for data that did not follow a normal distribution. All experiments were repeated three times, and differences were considered significant if the P-value < 0.05.
Flow cytometry data were analyzed using FlowJo 10.4.0 software. All images were assessed using ImageJ 1.53 software.
Results
ANXA10 is upregulated in the serrated pathway
To investigate the features of the serrated pathway, we conducted transcriptome sequencing (RNA-seq) on twelve pairs of SSL and corresponding NC. PCA analysis revealed significant differences between the SSL and NC groups (Fig. 1A). We performed differential analysis and identified differently expressed genes (DEG) using the |log2FoldChange|value > 1.5 and P < 0.05 criteria. ANXA10 was found to be significantly upregulated in SSL (Fig. 1B).
Given the high expression of ANXA10 in SSL, we further examined its expression levels in CRC patients. Analysis of the TCGA-COAD and GEO databases revealed that CRC patients with high ANXA10 expression had worse prognoses than those with low expression (P = 0.047) (Fig. 1C). In addition, ANXA10 expression was substantially higher in BRAF-mutated CRC (BRAFmut CRC) than in BRAF wild-type (BRAFwt CRC) (P < 0.0001; Fig. 1D, E). Furthermore, ANXA10 was expressed at higher levels in CRC located in the right colon than in the left (Fig. 1F, G), consistent with the fact that SSL and BRAF-mutated CRC occur more frequently in the right.
We also performed single-cell transcriptome sequencing of serrated lesions and discovered a subpopulation of epithelial cells specific to serrated lesions (Epi-SL) (Fig. 1H) [24]. Interestingly, ANXA10 was highly expressed in Epi-SL, while its expression was lower in normal subpopulations such as absorptive epithelium and cupped cells. Immunohistochemical staining revealed that ANXA10 was specifically upregulated in the crypt at the site of lesions in SSL and BRAFmut CRC (Fig. 1I).
Knockdown of ANXA10 represses viability and promotes the death of colorectal cancer cells
To investigate the impact of ANXA10 on CRC development, we analyzed the expression levels of ANXA10 mRNA in various CRC cell lines and found the highest expression in HT29 cells, followed by HCT116 and SW480 cells, and the lowest expression in RKO cells (Fig. 2A). To study the role of ANXA10 in CRC, we performed knockdown experiments of ANXA10 in HT29 and HCT116 cells and overexpression experiments in SW480 cells.
We used small-interfering RNAs (siRNAs) to knock down ANXA10 expression in HT29 and HCT116 cells, and siRNA-2 was identified as the most effective siRNA for ANXA10 knockdown, as confirmed by RT-PCR and Western blot analysis (Fig. S1A, B). Meanwhile, we transfected ANXA10-shRNA and control lentiviral plasmids into HT29 cells to construct ANXA10 knockdown (shANAX10) and control HT29 stable-transformed cell lines (shNC), respectively, and confirmed the knockdown efficiency by Western blot and RT-PCR analysis (Fig. S1C). Furthermore, we transiently transfected ANXA10 overexpression plasmids in SW480 and RKO cells and verified ANXA10 overexpression (Fig. S1D, E).
We then examined the effects of ANXA10 on cell survival and apoptosis. The viability of HT29 and HCT116 was significantly inhibited by ANXA10 siRNA (Fig. 2B, C), and a similar decrease in cell viability was observed in the HT29-shANXA10 stable-transformed cell line (Fig. 2D). Moreover, the knockdown of ANXA10 led to a significant increase in the proportion of early and late apoptotic cells (Fig. 2E, F and S2A, B), whereas ANXA10 overexpression in SW480 and RKO cells significantly decreased the percentage of apoptotic cells with or without cycloheximide (CHX) (Fig. 2G, H and S2C–H).
ANXA10 enhances the proliferation and migration of CRC cells
The CCK-8 assay showed that after the knockdown of ANXA10, HT29, and HCT116 cells proliferated significantly slower than the control group on days 3 and 4 (Fig. 3A, B). Furthermore, we observed that SW480 and RKO cells overexpressing ANXA10 proliferated substantially faster than the control cells (Fig. 3C, D).
Considering the association between high ANXA10 expression and poor prognosis in CRC patients, we speculated that ANXA10 might regulate the migration ability of CRC cells. Our results demonstrated that the knockdown of ANXA10 impaired the migratory ability of CRC cells (Fig. 3E, F), while overexpression of ANXA10 promoted their migration (Fig. 3G). Scratch assays also verified that overexpression of ANXA10 facilitated the ability of SW480 cells to heal scratches (Fig. 3H).
To further confirm the in vitro findings, we verified the migration ability of HT29-shANXA10 cells in vitro and found that it was significantly weaker than that of the control group (Fig. 3I, J). Subsequently, we established a lung metastasis model in nude mice by tail vein injection of HT29-shANXA10 or HT29-shNC cells. Eight weeks later, the mice were euthanized and found to have significantly fewer metastatic lesions in the lungs of the shANXA10-injected group compared to the control group, as confirmed by H&E staining (Fig. 3K–M).
Ferroptosis occurred in ANXA10 knockdown colorectal cancer cells
To elucidate the molecular mechanisms by which ANXA10 promotes malignant biological behaviors, such as survival, proliferation, and migration of CRC cells, we performed RNA-seq on HT29-shANXA10 and shNC cells. PCA reduced dimensional analysis revealed intergroup differences between the samples of the two groups, suggesting differences in transcriptome levels (Fig. 4A). Upon screening for DEG based on the criteria of differential expression fold (Fold-Change value) >2-fold or <0.5-fold and P < 0.05, we identified 153 genes with upregulated expression and 485 genes with down-regulated expression in the HT29-shANXA10 group compared to the control (Fig. 4B). KEGG pathway enrichment analysis on all up- and down-regulated genes revealed the ferroptosis pathway as the most significant among the top 15 pathways in terms of significance (P < 0.0001), along with other signaling pathways such as the Ras signaling pathway, arachidonic acid metabolism, NOD-like receptor signaling pathway, and Rap1 signaling pathway (Fig. 4C).
The considerable enrichment of the ferroptosis pathway prompted us to initiate a study on the role of ANXA10 in regulating this process. Lipid peroxidation and iron accumulation are two major biochemical features involved in ferroptosis. We, therefore, investigated the effect of knocking down ANXA10 on lipid peroxidation levels in CRC cells. Our results showed that after siRNA knockdown of ANXA10 in HT29 and HCT116 cells (siANXA10), the mean fluorescence intensity was significantly stronger detected by the liperfluo fluorescent probe compared to the control (P < 0.01 and P < 0.05, respectively; Fig. 4D, E, H, I). In addition, we also observed an increase in intracellular reactive oxygen species (ROS) levels in HT29 cells after ANXA10 knockdown using a DCFH-DA fluorescent probe (P < 0.01, Fig. 4F, G). These experimental results suggest that the lipid peroxidation and ROS levels were markedly increased after knocking down ANXA10 in CRC cells.
The primary products of lipid peroxidation include lipid peroxide (LOOH), malondialdehyde (MDA), and 4-hydroxynonenal (4HNE), and intracellular MDA concentration can indirectly reflect the degree of lipid peroxidation [25]. Our experimental results showed that the MDA concentration in the HT29-shANXA10 group was soaring ahead of the control (P < 0.01). Notably, treating cells with the ferroptosis inhibitor Ferrostatin-1 (Fer-1) for 48 h significantly reduced the MDA concentration in the shANXA10 group (P < 0.05), and there was no significant difference between the shANXA10 and control groups (Fig. 4J).
Glutathione (GSH) is the main intracellular antioxidant, and depletion of GSH exacerbates the accumulation of intracellular ROS, ultimately triggering ferroptosis [26]. Therefore, we further examined the ratio of reduced GSH to oxidized glutathione (GSSG) in cells. The results showed that the GSH/GSSG ratio was dramatically lower in the shANXA10 cohort than in the control group, while treatment with Fer-1 significantly restored the GSH/GSSG ratio in HT29-shANXA10 cells (Fig. 4K).
Subsequently, we detected the levels of Fe2+ in CRC cells using the FerroOrrange fluorescent probe. We found that the mean fluorescence intensity was more robust in the siANXA10 group than in the control (P < 0.001). After treating both groups of cells separately with the iron chelator, deferoxamine mesylate (DFO), for 48 h, we found that DFO dramatically reduced the mean fluorescence intensity of cells in the siANXA10 group (P < 0.0001, Fig. 4L, M). Therefore, we again examined Fe2+ levels in HT29 cells by flow cytometry and found experimental results consistent with those described above. Knockdown of ANXA10 resulted in a pronounced increase in intracellular mean fluorescence intensity (P < 0.01), while DFO significantly restored this trend (P < 0.01, Fig. 4N, O). Finally, we observed the fluorescence images of the FerroOrange probe inside the cells and noticed a distinct decrease in fluorescence intensity in the shANXA10 group of cells after DFO treatment (Fig. 4P).
Knockdown of ANXA10 inhibits autophagy-mediated TFRC degradation
To dissect the specific mechanisms underlying ferroptosis, we analyzed changes in ferroptosis-related genes in HT29 cells with ANXA10 knockdown. Ligase Catalytic Subunit (GCLC), Glutamate-Cysteine Ligase Modifier Subunit (GCLM), Solute Carrier Family 39 Member 14 (SLC39A14/Zip14), and Ceruloplasmin (CP) were elevated in HT29-shANXA10 cells, while SLC40A1 and SLC11A2/DMT1 were reduced (Fig. 5A). TFRC is a crucial bridge involved in translocating transferrin (TF)-bound iron (III) into cells [27]. Fe3+ entering the cell is reduced to Fe2+ by STEAP3, a metal reductase in the endosome, and then transported to the cytoplasm by SLC11A2. SLC40A1 is the primary channel for Fe2+ export from the cell membrane [28] while SLC39A14 is involved in the uptake of cellular non-transferrin-bound iron [29, 30].
To confirm the changes in iron ion transport-related genes, we examined their mRNA levels in HT29-shANXA10 and ANXA10-knockdown HCT116 cells (Fig. 5B and S3). qPCR results showed that the expression level of TFRC (P < 0.05 and P < 0.001 in HT29 and HCT116 cells, respectively), which mediates the inward flow of iron ions, was significantly increased in the ANXA10-knockdown groups of cells, whereas the expression levels of SLC40A1 (P < 0.05 in both HT29 and HCT116 cells), which translated the inward flow of iron ions, had slightly lower expression levels. Next, we investigated the expression levels of TFRC, an essential protein that is the dominant mode of iron uptake for cells. Western blot assays confirmed higher TFRC protein expression in HT29-shANXA10 cells than in shNC cells. However, the increase in TFRC expression was not restored after 48 h treatment with Fer-1 (1 μM) or DFO (200 μM) (Fig. 5C). The half-life of TFRC protein was significantly longer in HT29-shANXA10 cells than in shNC cells after inhibition of intracellular protein synthesis by cycloheximide (CHX) treatment (P < 0.05, Fig. 5D, E). Therefore, we speculate that increased levels of TFRC expression may be responsible for the ferroptosis that occurs in HT29-shANXA10 cells, and the knockdown of ANXA10 inhibits the degradation of TFRC protein in HT29 cells.
Research has revealed that TFRC degradation can occur through autophagy [31, 32], and based on this, we hypothesized that inhibiting autophagy-mediated degradation through the knockdown of ANXA10 may prevent the degradation of TFRC. To test our conjecture, we examined LC3B and autophagy receptor SQSTM1 protein levels. We found that HT29-shANXA10 cells accumulated significantly higher levels of LC3B compared to control cells, with no change in trend after treatment with either the autophagy inducer rapamycin (Rap) or the autophagy inhibitor chloroquine (CQ) (Fig. 5F). The protein expression level of SQSTM1 was significantly higher in HT29-shANXA10 cells than in the control group (Fig. 5F, G). The immunofluorescence analysis showed that TFRC was co-localized with the lysosomal marker LAMP1 in HT29 cells, but the co-localization of TFRC and LAMP1 decreased after ANXA10 knockdown (Fig. 5H). These results suggest that induction of autophagy partially restored TFRC degradation in HT29-shANXA10 cells, implying that knockdown of ANXA10 prevented TFRC degradation by inhibiting the autophagic process, especially the degradation of TFRC in the lysosome, thereby inducing ferroptosis in CRC cells (Fig. 6G).
To gain a more comprehensive understanding of the ANXA10-regulated protein profile, we performed mass spectrometry analysis on HT29-shANXA10 cells and controls. PCA analysis showed a distinguished difference in protein expression profiles between the two groups (Fig. 5I). Differentially expressed proteins (DEP) were screened according to the criteria of differential expression fold (Fold-Change value) >2-fold or <0.5-fold and P < 0.05. 46 proteins with upregulated expression and 40 with down-regulated expression were identified in the HT29-shANXA10 group compared to the control group (Fig. 5J). Correlation analysis of transcriptome and proteome sequencing results revealed that their changes were positively correlated after ANXA10 knockdown (Pearson r = 0.38, P < 0.001, Fig. 5J). Interestingly, SQSTM1 and TFRC were among the 33 genes with significant changes in both histological sequencing results (P < 0.05) (Fig. 5K), confirming that knockdown of ANXA10 led to the accumulation of SQSTM1 and suppression of TFRC degradation in CRC cells. Moreover, correlation analysis of transcriptomic and proteomic significantly enriched Hallmark pathways revealed that characteristic pathways such as tumor necrosis factor α (TNF-α)/NFκB signaling, apoptosis, Hedgehog signaling, protein secretion, and cholesterol homeostasis were significantly enriched in the shANXA10 group, while pathways such as interferon γ responsiveness, interferon α responsiveness, and bile acid metabolism were downmodulated (Fig. 5L).
Cell viability and migration were rescued by Ferrostatin-1 in ANXA10 knockdown colorectal cancer cells
Owing to the above observations, we hypothesized that the knockdown of ANXA10 induces ferroptosis in CRC cells by inhibiting autophagy-mediated TFRC degradation, thereby suppressing cell survival and migration ability. Our results demonstrated that treatment with Fer-1 restored the decreased cell viability of HCT116 and HT29 cells caused by ANXA10 knockdown (Fig. 6A, D), while having no significant effect on the survival of control cells. Fer-1 greatly improved the migration ability of ANXA10 knockdown HCT116 (Fig. 6B, C) and HT29 cells (Fig. 6E, F). These findings collectively showed that the ferroptosis inhibitor recovered the survival and migration capacity of knockdown ANXA10 CRC cells.
Discussion
ANXA10, a calcium-dependent phospholipid-binding protein, has been linked to poor survival in CRC [33] and an enhanced risk of developing heterochronic serrated lesions in individuals with serrated lesions [12]. This study is the first to investigate the expression and mechanisms of ANXA10 in the serrated carcinoma pathway of CRC. Consistent with previous studies, ANXA10 is specifically highly expressed in SSL and BRAFmut CRC and is associated with poor prognosis. single-cell sequencing and immunohistochemical assays confirmed that ANXA10 was predominantly expressed in epithelial cells with serrated lesions.
Research on ferroptosis is expanding and showing potential for the development of new therapeutic approaches for CRC. For example, salazosulfapyridine can induce ferroptosis by inhibiting the cell membrane cystine glutamate transporter receptor (System Xc-) and depleting GSH, which promotes sensitivity to cisplatin in CRC [34]. Dimethyl fumarate induces ferroptosis in CRC cells by depleting GSH, increasing ROS, and activating MAPK [35]. Targeting ferroptosis can enhance the therapeutic effect of CRC, improve sensitivity to radiotherapy, and reduce cellular resistance [36]. Our study found that knockdown of ANXA10 induced ferroptosis in CRC cells, suggesting that ANXA10 is an effective target for inducting ferroptosis in the treatment of ANXA10 highly expressed CRC.
Iron deficiency in CRC has been linked to a less favorable prognosis and poor treatment response [37, 38]. Therefore, increasing the concentration of Fe2+ in CRC cells is expected to improve the prognosis of CRC patients. Our study revealed that knockdown of ANXA10 inhibited the degradation of TFRC, resulting in a significant increase in intracellular Fe2+ concentration and inducing ferroptosis in CRC cells. Thus, it is possible to significantly inhibit cell growth by up-regulating the concentration of iron ions in ANXA10 highly expressed CRC cells.
In our study, we observed a distinct increase in autophagic flux and accumulation of SQSTM1 following knockdown of ANXA10, which ultimately hindered the autophagic process in CRC cells, suggesting that ANXA10 plays a role in the autophagy process. This biological function is similar to other proteins of the membrane-linked protein A family [11], such as ANXA2, which promotes the formation of autophagosomes and mediates the fusion of autophagosomes and lysosomes [39, 40]. The role played by ANXA10 in the autophagic process warrants further investigation.
While our findings showed that the knockdown of ANXA10 induced ferroptosis and hindered the malignant proliferation and migration of CRC cells, it remains unclear whether the ferroptosis triggered by ANXA10 downregulation can enhance the sensitivity of existing chemotherapy, targeted therapy, or immunotherapy regimens. Therefore, it is necessary to conduct cellular and animal-level experiments to demonstrate the efficacy of ANXA10 knockdown in combination with other therapeutic regimens. In addition, further studies should focus on the mechanisms by which ANXA10 affects TFRC degradation in lysosomes and understand how ANXA10 regulates the autophagy cycle.
This study provides strong evidence that ANXA10 is significantly upregulated in patients with SSL and BRAF mutant CRC, and is strongly associated with poor prognosis. Our results indicate that knockdown of ANAX10 can inhibit the malignant capacity of colorectal cancer cells by inhibiting autophagy-mediated degradation of TFRC, leading to cellular ferroptosis. The ANXA10–TFRC–ferroptosis axis sheds light on a novel therapy for CRC originating from the serrated pathway. Further exploration of this axis could potentially lead to the development of more effective treatment options for this subtype of CRC, ultimately improving patient outcomes.
Data availability
The datasets generated during the current study are available in the NIH National Center for Biotechnology Information Sequence Read Archive (SRA) repository, http://www.ncbi.nlm.nih.gov/bioproject/950129 and Supplementary Table S3.
Change history
16 October 2023
A Correction to this paper has been published: https://doi.org/10.1038/s41419-023-06151-x
References
Sung H, Ferlay J, Siegel RL, Laversanne M, Soerjomataram I, Jemal A, et al. Global Cancer Statistics 2020: GLOBOCAN Estimates of Incidence and Mortality Worldwide for 36 Cancers in 185 Countries. Cancer J Clin. 2021;71:209–49.
Leggett B, Whitehall V. Role of the serrated pathway in colorectal cancer pathogenesis. Gastroenterology. 2010;138:2088–100.
Longacre TA, Fenoglio-Preiser CM. Mixed hyperplastic adenomatous polyps/serrated adenomas. A distinct form of colorectal neoplasia. Am J Surg Pathol. 1990;14:524–37.
Crockett SD, Nagtegaal ID. Terminology, molecular features, epidemiology, and management of serrated colorectal neoplasia. Gastroenterology. 2019;157:949–66.e4.
Nagtegaal ID, Odze RD, Klimstra D, Paradis V, Rugge M, Schirmacher P, et al. The 2019 WHO classification of tumours of the digestive system. Histopathology. 2020;76:182–8.
Oono Y, Fu K, Nakamura H, Iriguchi Y, Yamamura A, Tomino Y, et al. Progression of a sessile serrated adenoma to an early invasive cancer within 8 months. Dig Dis Sci. 2009;54:906–9.
Amemori S, Yamano H-O, Tanaka Y, Yoshikawa K, Matsushita H-O, Takagi R, et al. Sessile serrated adenoma/polyp showed rapid malignant transformation in the final 13 months. Dig Endosc. 2020;32:979–83.
Murakami T, Sakamoto N, Nagahara A. Endoscopic diagnosis of sessile serrated adenoma/polyp with and without dysplasia/carcinoma. World J Gastroenterol. 2018;24:3250–9.
De Palma FDE, D’Argenio V, Pol J, Kroemer G, Maiuri MC, Salvatore F. The molecular hallmarks of the serrated pathway in colorectal cancer. Cancers (Basel). 2019;11:1017.
Tao Y, Kang B, Petkovich DA, Bhandari YR, In J, Stein-O'Brien G. et al. Aging-like spontaneous epigenetic silencing facilitates Wnt activation, stemness, and BrafV600E-induced tumorigenesis. Cancer Cell. 2019;35:315–28.e6.
Xi Y, Ju R, Wang Y. Roles of Annexin A protein family in autophagy regulation and therapy. Biomed Pharmacother. 2020;130:110591.
Macaron C, Lopez R, Pai RK, Burke CA. Expression of annexin A10 in serrated polyps predicts the development of metachronous serrated polyps. Clin Transl Gastroenterol. 2016;7:e205.
Gonzalo DH, Lai KK, Shadrach B, Goldblum JR, Bennett AE, Downs-Kelly E, et al. Gene expression profiling of serrated polyps identifies annexin A10 as a marker of a sessile serrated adenoma/polyp. J Pathol. 2013;230:420–9.
Kim JH, Kim K-J, Rhee Y-Y, Bae JM, Cho N-Y, Lee HS, et al. Gastric-type expression signature in serrated pathway-associated colorectal tumors. Hum Pathol. 2015;46:643–56.
Sajanti SA, Väyrynen JP, Sirniö P, Klintrup K, Mäkelä J, Tuomisto A, et al. Annexin A10 is a marker for the serrated pathway of colorectal carcinoma. Virchows Arch. 2015;466:5–12.
Kim JH, Rhee Y-Y, Kim K-J, Cho N-Y, Lee HS, Kang GH. Annexin A10 expression correlates with serrated pathway features in colorectal carcinoma with microsatellite instability. APMIS. 2014;122:1187–95.
Zhang X, Hu Z, Wang X, Li L, Zhu B, Lin X, et al. ANXA10 promotes melanoma metastasis by suppressing E3 ligase TRIM41-directed PKD1 degradation. Cancer Lett. 2021;519:237–49.
Sun R, Liu Z, Qiu B, Chen T, Li Z, Zhang X, et al. Annexin10 promotes extrahepatic cholangiocarcinoma metastasis by facilitating EMT via PLA2G4A/PGE2/STAT3 pathway. EBioMedicine. 2019;47:142–55.
Kodaira H, Koma Y-I, Hosono M, Higashino N, Suemune K, Nishio M, et al. ANXA10 induction by interaction with tumor-associated macrophages promotes the growth of esophageal squamous cell carcinoma. Pathol Int. 2019;69:135–47.
Shimizu T, Kasamatsu A, Yamamoto A, Koike K, Ishige S, Takatori H, et al. Annexin A10 in human oral cancer: biomarker for tumoral growth via G1/S transition by targeting MAPK signaling pathways. PLoS ONE. 2012;7:e45510.
Zhuang C, Wang P, Sun T, Zheng L, Ming L. Expression levels and prognostic values of annexins in liver cancer. Oncol Lett. 2019;18:6657–69.
Miyazawa Y, Sekine Y, Kato H, Furuya Y, Koike H, Suzuki K. Simvastatin Up-regulates annexin A10 that can inhibit the proliferation, migration, and invasion in androgen-independent human prostate cancer cells. Prostate. 2017;77:337–49.
Munksgaard PP, Mansilla F, Brems Eskildsen A-S, Fristrup N, Birkenkamp-Demtröder K, Ulhøi BP, et al. Low ANXA10 expression is associated with disease aggressiveness in bladder cancer. Br J Cancer. 2011;105:1379–87.
Zhou Y-J, Lu X-F, Chen H, Wang X-Y, Cheng W, Zhang Q-W, et al. Single-cell transcriptomics reveals early molecular and immune alterations underlying the serrated neoplasia pathway toward colorectal cancer. Cell Mol Gastroenterol Hepatol. 2023;15:393–424.
Tang D, Chen X, Kang R, Kroemer G. Ferroptosis: molecular mechanisms and health implications. Cell Res. 2021;31:107–25.
Dixon SJ, Lemberg KM, Lamprecht MR, Skouta R, Zaitsev EM, Gleason CE, et al. Ferroptosis: an iron-dependent form of nonapoptotic cell death. Cell. 2012;149:1060–72.
Feng H, Schorpp K, Jin J, Yozwiak CE, Hoffstrom BG, Decker AM, et al. Transferrin receptor is a specific ferroptosis marker. Cell Rep. 2020;30:3411–23.e7.
Montalbetti N, Simonin A, Kovacs G, Hediger MA. Mammalian iron transporters: families SLC11 and SLC40. Mol Asp Med. 2013;34:270–87.
Zhao N, Zhang A-S, Wortham AM, Jue S, Knutson MD, Enns CA. The tumor suppressor, P53, decreases the metal transporter, ZIP14. Nutrients. 2017;9:1335.
Pinilla-Tenas JJ, Sparkman BK, Shawki A, Illing AC, Mitchell CJ, Zhao N, et al. Zip14 is a complex broad-scope metal-ion transporter whose functional properties support roles in the cellular uptake of zinc and nontransferrin-bound iron. Am J Physiol Cell Physiol. 2011;301:C862–71.
Xiong Q, Li X, Li W, Chen G, Xiao H, Li P, et al. WDR45 mutation impairs the autophagic degradation of transferrin receptor and promotes ferroptosis. Front Mol Biosci. 2021;8:645831.
Shan J, Jiang W, Chang J, Zhou T, Chen Y, Zhang Y, et al. NUF2 drives cholangiocarcinoma progression and migration via inhibiting autophagic degradation of TFR1. Int J Biol Sci. 2023;19:1336–51.
Bae JM, Kim JH, Rhee Y-Y, Cho N-Y, Kim T-Y, Kang GH. Annexin A10 expression in colorectal cancers with emphasis on the serrated neoplasia pathway. World J Gastroenterol. 2015;21:9749–57.
Ma M-Z, Chen G, Wang P, Lu W-H, Zhu C-F, Song M, et al. Xc- inhibitor sulfasalazine sensitizes colorectal cancer to cisplatin by a GSH-dependent mechanism. Cancer Lett. 2015;368:88–96.
Xie X, Zhao Y, Ma C-Y, Xu X-M, Zhang Y-Q, Wang C-G, et al. Dimethyl fumarate induces necroptosis in colon cancer cells through GSH depletion/ROS increase/MAPKs activation pathway. Br J Pharm. 2015;172:3929–43.
Wang Y, Zhang Z, Sun W, Zhang J, Xu Q, Zhou X, et al. Ferroptosis in colorectal cancer: Potential mechanisms and effective therapeutic targets. Biomed Pharmacother. 2022;153:113524.
Aksan A, Farrag K, Aksan S, Schroeder O, Stein J. Flipside of the coin: iron deficiency and colorectal cancer. Front Immunol. 2021;12:635899.
Phipps O, Brookes MJ, Al-Hassi HO. Iron deficiency, immunology, and colorectal cancer. Nutr Rev. 2021;79:88–97.
Morozova K, Sridhar S, Zolla V, Clement CC, Scharf B, Verzani Z, et al. Annexin A2 promotes phagophore assembly by enhancing Atg16L+ vesicle biogenesis and homotypic fusion. Nat Commun. 2015;6:5856.
Bustos V, Pulina MV, Bispo A, Lam A, Flajolet M, Gorelick FS, et al. Phosphorylated presenilin 1 decreases β-amyloid by facilitating autophagosome-lysosome fusion. Proc Natl Acad Sci USA. 2017;114:7148–53.
Acknowledgements
We are grateful to all the individuals who participated in the study.
Funding
This work was supported by the Health and Family Planning Research Project of the Shanghai Pudong New Area Health Commission (PW2020D-12).
Author information
Authors and Affiliations
Contributions
XBL conceptualized and supervised the study; XYW and YJZ collected the samples and analyzed the data; XYW and LJN performed the investigation and experiments; XYW and JNC drafted the manuscript; XBL and HMC reviewed and edited the manuscript.
Corresponding author
Ethics declarations
Competing interests
The authors declare no competing interests.
Ethics approval and consent to participate
This study was approved by the Ethics Committee of Shanghai Renji Hospital. All study participants provided informed written consent before study enrollment.
Additional information
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Wang, X., Zhou, Y., Ning, L. et al. Knockdown of ANXA10 induces ferroptosis by inhibiting autophagy-mediated TFRC degradation in colorectal cancer. Cell Death Dis 14, 588 (2023). https://doi.org/10.1038/s41419-023-06114-2
Received:
Revised:
Accepted:
Published:
DOI: https://doi.org/10.1038/s41419-023-06114-2