Background
Resistance is associated with or promotes a highly aggressive phenotype [
1]. One common mechanism is that cancer cells can evolve additional capabilities, such as enhanced invasion and metastasis with the acquisition of resistance. These abilities are often associated with reprogramming of intracellular gene expression and activation of the corresponding intracellular signaling pathways [
2‐
5]. For instance, metastasis-related proteins are often upregulated in drug-resistant cells [
1,
2,
6‐
8]; chronic anticancer drug treatments often induce epithelial-to-mesenchymal transition in tumor cells, a phenotypic change that is closely related to metastasis [
9‐
11]. Therefore, the drug resistance of cancer cells not only leads to treatment failure, but may also result in rapid recurrence and metastasis. Thus, determining the molecular mechanisms governing the aggressive behavior of drug-resistant tumors is critical for designing highly effective therapeutic strategies.
Recent studies have revealed several key molecules involved in the development of drug resistance and associated signal pathways responsible for cancer progression [
2,
12]. One molecule is Annexin A2 (Anxa2), a calcium-dependent phospholipid-binding protein [
2,
12‐
14]. Anxa2 has been shown as a multifunctional protein implicated in many biological processes [
13‐
15]. Its abnormal expression is associated with a variety of diseases, especially cancer [
13‐
15]. Anxa2 overexpression promotes proliferation, migration, invasion, angiogenesis, and metastasis in various types of tumors [
13‐
15]. In addition, a high Anxa2 level has been observed in many types of drug-resistant cells [
16‐
20]. The increased expression of Anxa2 in these cells not only confers resistance to anticancer agents, but also enhances their aggressive behavior [
18,
21,
22]. Moreover, clinical studies have shown that Anxa2 overexpression is positively correlated to poor response to anticancer agents and rapid recurrence in cancer patients who had received chemotherapy [
21,
23‐
25]. This evidence suggests that Anxa2 is a key protein that links drug resistance and cancer metastasis. Therefore, uncovering the detailed mechanisms through which Anxa2 promotes cancer progression is urgently required.
The biological function of Anxa2 is modulated by post-translational modifications, including phosphorylation, acetylation, ubiquitination, and sumoylation [
13,
15,
26]. Anxa2 can be phosphorylated at Tyr23 by Src-family tyrosine kinase in response to growth factors, such as epidermal growth factor (EGF) and platelet-derived growth factor (PDGF) [
13]. In addition, Anxa2 Tyr23 phosphorylation (pY23-Anxa2) has been found to be upregulated in response to anticancer drugs, including genotoxic agents and microtubule interfering agents [
12,
27]. pY23-Anxa2 is involved in the promotion of invasion and metastasis in cancer cells and associated with disease progression in cancer patients [
13,
15]. Nevertheless, little information is available concerning the regulatory mechanism of Anxa2 tyrosine phosphorylation, and whether the phosphorylation is necessary for the enhanced invasive phenotype of drug-resistant cells remains unknown.
We have previously demonstrated that the receptor for activated protein C kinase 1 (Rack1) is a novel binding protein of Anxa2 [
28]. Rack1 acts as a multifaceted scaffold protein that is involved in various cellular activities by mediating protein–protein interactions [
29,
30]. The function of Rack1 on cancer progression is cancer type-specific [
29‐
31]. Except for colon and gastric cancer [
32‐
34], Rack1 appears to play a tumor-promoting role in other carcinomas [
29‐
31]. Additionally, Rack1 overexpression has been correlated to proliferation, invasion, and metastasis [
35‐
38]. In particular, higher Rack1 level is an independent predictor for poor prognosis in breast cancer. Recently, Rack1 has been reported to be a key protein involved in drug resistance in several carcinomas [
39‐
43]. These findings have suggested that Rack1 may act as an important convergence point for drug resistance and invasion/metastasis. We previously reported that Rack1 is required for the migration and invasion potential of drug-resistant breast cancer cells [
28]. We demonstrated that Rack1 acts as a molecular bridge mediating the binding of Src and Anxa2 to P-glycoprotein. Interestingly, Rack1 is also a binding protein of Src kinase [
30]. Rack1 knockdown decreases Adriamycin-triggered Tyr23 phosphorylation of Anxa2 in drug-resistant breast cancer [
28]. However, the detailed mechanism by which Rack1 regulates Anxa2 phosphorylation remains unclear. The accurate function of Rack1 in promoting the aggressive behavior in drug-resistant breast cancer cells has not been thoroughly determined. In this work, we further explored the effect of Rack1 on the invasive and metastatic potential in drug-resistant breast cancer cells, and investigated the mechanism underlying the regulation of Anxa2 Tyr23 phosphorylation. We showed that Rack1 and Anxa2 are required for the invasive and metastatic potential of multidrug-resistant (MDR) breast cancer cells. Rack1 mediates Anxa2 binding to Src, thereby facilitating Anxa2 phosphorylation by Src. Our findings suggest that the interaction between Anxa2 and Rack1/Src is responsible for the association between drug resistance and aggressive behavior in breast cancer cells.
Materials and methods
Antibodies, reagents, and drugs
The following antibodies, reagents, and drugs were used: DMEM/F12, RPMI 1640, DMEM/High glucose medium and trypsin (Hyclone, Logan, UT, USA); Fetal Bovine Serum (FBS, Gibco, Carlsbad, CA, USA); Src inhibitor KX2-391 (Selleckchem, Houston, TX, USA); transwell inserts (Corning Inc., Corning, NY, USA); EGF (Cat No. 236-EG, R&D, USA); Matrigel (BD Biosciences, San Jose, CA, USA); Protein A/G agarose beads (Invitrogen, Carlsbad, CA, USA); Lipofectamine RNAiMax and Lipofectamine 2000 (Invitrogen, Carlsbad, CA, USA); antibodies against Rack1 (sc-17754), Anxa2 (sc-28385), p-Anxa2 (sc-135753), GFP (sc-9996, Santa Cruz Biotechnology, Santa Cruz, CA, USA); antibodies against Src (# 2123) and p-Src (# 6943, Cell Signaling Technology, Beverly, MA, USA); antibodies against Flag (F1804) and β-actin (A1978, Sigma, St. Louis, MO, USA); and Rack1, Anxa2, and Src small interfering RNAs (siRNAs, Invitrogen, Carlsbad, CA, USA, detailed information is listed in Table
1).
Table 1
siRNA sequences used in this study
siRack1-1# | Upper: UAUCUCGAGAUCCAGAGACAAUCUG |
Lower: CAGAUUGUCUCUGGAUCUCGAGAUA |
siRack1-2# | Upper: ACGAUGAUAGGGUUGCUGCUGUUGG |
Lower: CCAACAGCAGCAACCCUAUCAUCGU |
siSrc-1# | Upper: CAGCAGCUGGUGGCCUACUACUCCA |
Lower: UGGAGUAGUAGGCCACCAGCUGCUG |
siSrc-2# | Upper: GAGCCCAAGCUGUUCGGAGGCUUCA |
Lower: UGAAGCCUCCGAACAGCUUGGGCUC |
siAnxa2-1# | Upper: UACAGCAGCGCUUUCUGGUAGUCGC |
Lower: GCGACUACCAGAAAGCGCUGCUGUA |
Cell culture and siRNA transfection
Human triple-negative breast cancer (TNBC) MDA-MB-468 cells were obtained from American Type Culture Collection (ATCC). The drug-resistant variant cell line MDA-MB-468/EPR was established by our group using a stepwise exposure to an increasing concentration of epirubicin. The human luminal-type breast cancer MCF-7 cells and its drug-resistant cell line MCF-7/ADR was kindly provided by Dr. Zizheng Hou (Henry Ford Hospital, Detroit, MI, USA). Anxa2 stably silenced MCF-7/ADR and control cells have been established in our previous study [
18]. HEK-293T cells were obtained from ATCC. The following media supplemented with 10% FBS were used for cell culture: DMEM/F12 for MDA-MB-468/EPR, modified RPMI-1640 for MCF-7/ADR, and DMEM/High glucose for HEK-293T. For siRNA transfection, cells were seeded into six-well plates and cultured to 30–40% confluence. Afterwards, control, Rack1-, Anxa2-, and Src-specific siRNAs were transfected using Lipofectamine RNAiMAX reagent according the manufacturer’s instructions.
Vector construction, lentivirus production, and infection
Flag-tagged, full-length, and wild-type Rack1 (Rack1WT) was generated by polymerase chain reaction (PCR) amplification with the following primers: upper: 5′-GAGAGCTAGCATGACTGAGCAGATGACCCT-3′, lower: 5′- GAGAGCGGCCGCCTACTTGTCGTCATCGTCTTTGTAGTCGCGTGTGCCAATGG-3′. Afterwards, the Rack1-coding region was cloned into a lentiviral vector pCDH-hygromycin in the Nhe I and Not I cloning sites. The Rack1Y246F mutant was generated by mutating the codon TAC (Y) of its amino acid 246 to TTC (F), where tyrosine 246 was replaced by phenylalanine. For Rack1 stable knockdown, a validated siRNA sequence targeting the Rack1 non-coding region (5′-TGGCACACGCTAGAAGTTTATGG-3′) was cloned into the lentiviral vector pLKO.1-hygromycin of the BamH I and Age I cloning sites. The lentiviral plasmids pCDH-Anxa2WT-GFP, pCDH-Anxa2Y23A-GFP, and pCDH-Anxa2Y23D-GFP were obtained in our previous study. In brief, wild-type Anxa2 (Anxa2WT) was generated by PCR amplification with the following primers: upper: 5′-CGGCTCGAGATGTCTACTGTTCACGAAATCCTG-3′, lower: 5′-CGTGGATCCGTCATCTCCACCACACAG-3′. Afterwards, the Anxa2-coding region was cloned into pEGFP-N3 vector in the Xho I and BamH I cloning sites. Anxa2Y23A-GFP and Anxa2Y23D-GFP mutants were generated by mutating the codon TAT (Y) of its amino acid 23 to GCT (A) or GAT (D). Then, the Anxa2-GFP fragments were further subcloned into the lentiviral vector pCDH-hygromycin in the Nhe I and Not I cloning sites. All constructs were confirmed by double-enzyme digestion and DNA sequencing. Lentivirus production was performed as described previously by using a three-plasmid packaging system. In brief, HEK-293T cells were plated in 10-cm dish and cultured to 60% confluence. Afterwards, the cells were co-transfected with the lentiviral plasmid and two packaging plasmids. The virus in the supernatants were collected, concentrated, and used to infect target cells 48 h after transfection. Stable cell lines were selected by using 50 μg/mL of hygromycin B.
Western blot and co-immunoprecipitation assay
Western blot assay was performed as described previously [
44]. Briefly, the cells were lysed with 1× SDS lysis buffer; the cell lysates after protein quantification were used for SDS-PAGE separation and subsequently transferred to a PVDF membrane. The membranes were blocked by 5% non-fat milk and probed with corresponding primary antibodies. After washing with 1× TBST, the membrane was incubated with horseradish peroxidase-labeled secondary antibodies, and the signals were subsequently detected using the ECL kit. β-actin was used as a loading control. For EGF-induced Anxa2 phosphorylation assay, control, Rack1, or Src siRNA transfected cells were starved for 8 h. Then, the cells were stimulated with 10 ng/mL of EGF for 0, 5, and 10 min. The cells were lysed, and the total cellular protein was analyzed by using Western blotting analysis. Co-IP assay was performed as described previously [
28]. Briefly, MCF-7/ADR and MDA-MB-468/EPR cells were transfected with negative control, Src-, Anxa2-, or Rack1-specific siRNAs for 72 h. Then, the cells were lysed with Tris-Trion X100-based lysis buffer. Afterwards, the quantified cell lysates were pre-cleared with protein G-linked agarose beads, followed by incubation with corresponding antibodies (Anxa2, Rack1, or Src) to enrich immunocomplex. The interacting proteins were captured with Protein A/G conjugated beads and subsequently analyzed by Western blotting with anti-Anxa2, Rack1, or Src antibodies.
Wound healing and transwell assay
Wound healing assay was carried out as described previously [
12]. The control and experimental cells were planted in six-well plates and grown to confluence. Afterward, a wound was prepared by scraping the cell monolayer using a 10-μL pipette tip. Afterward, the cells were incubated at 37 °C in a medium containing 0.5% FBS, and the cells were allowed to migrate for 0, 12, 24, 36, 48, and 60 h. The wound areas were photographed under an inverted microscope in indicated times, and the relative migrated distance was calculated with ImageJ. Transwell assays were performed by using Boyden chambers with a 8-μm filter pore. For migration assay, 1 × 10
5 cells in 200 μL serum-free medium were loaded into the upper chamber. The lower chamber was loaded with 600 μL of 10% FBS-containing medium. After incubation at 37 °C for 16 h, the migrated cells were fixed, stained, and quantified at 200×. For invasion assay, 2.5 × 10
5 cells were loaded into the upper insert coated with Matrigel, and the incubation time was 24 h. To examine the effect of Src inhibitors on migration and invasion of drug-resistant cells, the cells were pre-treated with Src inhibitors for 2 h. Then, transwell assays were performed in the absence (for migration) or presence (for invasion) of Matrigel.
Six-week-old female SCID mice were purchased from Beijing Charles River. All operations followed the guidelines approved by the Animal Ethical and Welfare Committee of Tianjin Medical University Cancer Institute and Hospital. For metastasis assay, control and Rack1 stably silenced cells, as well as the Rack1 rescued cells, were cultured to log phase. Then, the cells were trypsinized, washed thrice with PBS, resuspended, and adjusted to a concentration of 2 × 107 cells/mL. 2 × 106 cells (n = 8 per group) were injected into SCID mice via tail veins. Three months after injection, the mice were sacrificed; the lungs were dissected, fixed with formalin, embedded in paraffin, and serially sectioned. After hematoxylin and eosin staining, the micrometastasis foci in lungs were visualized and counted under a microscope.
Immunofluorescence staining and apoptosis assay
Standard protocols are detailed in Additional file
1: Supplementary methods.
Statistical analysis
All data were shown as mean ± SD. The statistical differences were analyzed using the GraphPad Prism 7.00 software (GraphPad Software, La Jolla, CA, USA). For multiple sets of comparisons, one-way or two-way ANOVA was performed. P values less than 0.01 (two-tailed) were considered statistically significant. *indicates that the P value is less than 0.01 and ** means P value is less than 0.001.
Discussion
A high level of Anxa2 in cancer tissues is correlated with a highly aggressive phenotype [
15,
46,
48‐
51]. Increased Anxa2 expression has been shown to be specific in many drug-resistant cancer cells [
2,
16‐
20]. Moreover, recent studies have shown that Anxa2 is a key protein that links drug resistance and cancer metastasis [
2,
12,
15]. The functional activity of Anxa2 has been shown to be regulated by tyrosine phosphorylation at the Tyr23 site [
13]. Nevertheless, the accurate molecular mechanisms underlying the regulation of Anxa2 tyrosine phosphorylation and whether phosphorylation is necessary for the enhanced invasive phenotype of drug-resistant cells remain unknown. In this study, we demonstrated that Anxa2 Tyr23 phosphorylation is required for MDR breast cancer invasion and metastasis. Anxa2 functions downstream of Rack1/Src complex, and Rack1 is required for EGF-induced tyrosine phosphorylation of Anxa2, as well as the migration and invasion abilities in drug-resistant cells. Moreover, we provided evidence that Rack1 acts as a signal hub and mediates the interaction between Src and Anxa2, thereby facilitating Anxa2 phosphorylation by Src kinase. Hence, our findings suggest a new role of Rack1 in regulating Anxa2 tyrosine phosphorylation.
Elevated Anxa2 expression seems a common event when cancer cells acquire drug resistance (Additional file
2: Figure S5 A and C) [
2,
16‐
20,
45,
52,
53]. Anxa2 overexpression promotes chemoresistance in non-small cell lung cancer, pancreatic cancer, neuroblastoma, and hepatocarcinoma [
16,
17,
54,
55]. Moreover, Anxa2 confers increased invasiveness in breast cancer (Additional file
2: Figure S5 B and C) [
18,
56,
57]; Anxa2 knockdown also inhibits migration and invasion in nasopharyngeal carcinoma [
21,
22]. However, whether Anxa2 expression per se or its phosphorylated form confers the aggressive phenotype of drug-resistant cells remains unclear. We observed that the reduction of phosphorylated Anxa2 was associated with decreased invasiveness in MDR breast cancer cells. In addition, re-expression of phospho-mimicking Anxa2
Y23D, but not the phospho-deficient Anxa2
Y23A mutant, in Anxa2-silenced cells restored cell invasive potential. Expression of Anxa2
Y23D even showed an increased invasion ability compared with that of Anxa2
WT-expressing cells. These results suggested a functional association between Anxa2 Tyr23 phosphorylation and invasive behavior in resistant cells. Several studies have shown that chemotherapeutic agents can enhance phosphorylation of Anxa2 in cancer cells [
12,
27], and anti-cancer drugs have been shown to induce highly aggressive phenotypes in resistant cells [
9,
11,
58]. Additionally, phosphorylated Anxa2 confers resistance in several cancer cells [
45,
59]. Consistent with other studies, we have proven that Anxa2 Tyr23 phosphorylation is critical in the invasion and metastasis of many types of cancer [
48,
56,
60]. These results indicated that increased Anxa2 Tyr23 phosphorylation can be a mechanism for drug-resistant cells to enhance its migration and invasion abilities.
To date, the precise mechanism regulating Anxa2 Tyr23 phosphorylation remains largely unknown. We previously showed that the scaffold protein Rack1 binds Anxa2 and regulates Adriamycin-induced phosphorylation of Anxa2 [
28]. Rack1 knockdown inhibits basal level and EGF-induced phosphorylation of Anxa2 in drug-resistant cells, thus suggesting that Rack1 is a key molecule that modulates Anxa2 phosphorylation. Src is the major kinase that phosphorylates Anxa2 in many types of cells, and the blockage of Src activity with inhibitors or siRNAs inhibits phosphorylated Anxa2 in two resistant cells. Rack1 is known as a signaling bridge mediating protein–protein interaction [
30]. These data raised a possibility that Rack1 may nucleate a complex with Src and Anxa2, thereby facilitating Anxa2 phosphorylation by Src. Rack1 knockdown notably attenuated the binding of Src to Anxa2, whereas silencing the expression of Anxa2 or Src does not affect their interaction with Rack1, demonstrating that Rack1 mediates the interaction between Src and Anxa2. Consistently, our finding showed that re-expression of Rack1
WT, not the Src binding-deficient Rack1
Y246F mutant, in Rack1-silenced cells restored Anxa2 phosphorylation; this finding further confirmed this hypothesis. Taken together, our results suggest that Rack1 modulates Anxa2 tyrosine phosphorylation through a Src-dependent manner. To our knowledge, this study is the first to demonstrate the regulatory mechanism of Anxa2 phosphorylation by Rack1.
Deregulated expression of Rack1 has been reported in many types of carcinoma, and the function of Rack1 on cancer invasion and metastasis appears cancer type- and cell context-specific [
29,
30]. Rack1 inhibits the invasion ability of colon cancer cells [
33]. Moreover, Rack1 negatively regulates the invasiveness and metastasis of cancer cells in gastric cancer [
32,
34]; On the contrary, Rack1 promotes invasion and metastasis of prostate cancer and hepatocellular carcinoma cells [
61,
62]; Consistently, knockdown of Rack1 reduces invasion in melanoma, oral squamous carcinoma cells, and lung cancer cells [
35,
36,
38,
63]. In this study, silencing Rack1 in drug-resistant cells inhibited invasion ability in vitro and metastasis potential in vivo. Thus, our results support the tumor-promoter role of Rack1 in breast cancer. These data were in line with previous studies, showing that Rack1 promotes aggressive behavior in breast cancer [
64,
65]. Interestingly, recent studies have shown that Rack1 also confers resistance to cancer. Rack1 elevation enhances chemoresistance in leukemia, hepatocellular carcinoma, and esophageal cancer [
39,
41,
43]; Rack1 overexpression promotes targeted therapy resistance in gastrointestinal stromal tumor [
42]. These findings indicate that Rack1 might also be a critical hub involved in the crosstalk between drug resistance and invasion/metastasis. We proposed that Anxa2 functions downstream of Rack1 to promote the aggressive behavior in drug-resistant cells given that Rack1 binds and regulates Anxa2 phosphorylation, and Anxa2 is a key protein causing drug resistance and enhancement of cancer metastasis [
2]. In support of this hypothesis, exogenous expression of Anxa2
WT or Anxa2
Y23D instead of Anxa2
Y23A mutant notably rescued the migration and invasion defects in Rack1-silenced cells. These data suggest that Anxa2 mediates the biological function of Rack1/Src in drug-resistant breast cancer cells.
Although we have demonstrated the critical role of the Rack1/Src/Anxa2 complex in promoting aggressive behavior of drug-resistant cells, the accurate molecular mechanisms downstream of the complex remain to be determined. We have reported that pY23-Anxa2 binds to and enhances STAT3 activation and promotes invasion and metastasis of breast cancer cells [
56]. Consistently, Anxa2 associates with STAT3 and confers the aggressive behavior in colorectal cancer [
46,
66]. Interestingly, Rack1 is also involved in the activation of STAT3 in several cancer cells [
36,
67]. Src is also a well-known upstream kinase of STAT3, and enhanced STAT3 activation confers invasiveness of drug-resistant breast cancer cells [
8]. Therefore, these findings suggest that a possible downstream pathway of the Rack1/Src/Anxa2 complex may involve STAT3 signaling. In addition, another mechanism by which this complex promotes tumor invasion and metastasis may be through regulation of actin remodeling, which is essential for the migration and invasion of cancer cells. It has been reported that pY23-Anxa2 is involved in the regulation of Rho-mediated actin rearrangement [
51,
60,
68,
69]. Interestingly, Rack1 also interacts with Rho and activates RhoA/Rho kinase pathway to enhance breast cancer metastasis [
64]. Moreover, several studies have shown that pY23-Anxa2 promotes cancer cell invasion and metastasis through enhancing epithelial-mesenchymal transition (EMT) [
46,
60,
70]. Likewise, Rack1 has also been reported to regulate EMT and contribute cancer metastasis [
71,
72]. Drug-resistant cells are always associated with EMT phenotype [
73‐
75]. Hence, EMT may also be a possible mechanism for Rack1/Src/Anxa2 complex to promote the malignant behavior of drug-resistant cells. In future studies, it will be interesting to delineate the detailed mechanism by which this complex promotes invasion and metastasis of drug-resistant cells.