Both epithelial–mesenchymal transition (EMT) and mesenchymal–epithelial transition (MET) are linked to metastasis via their ability to increase invasiveness and enhance tumor-initiating capacity. Growth factors, cytokines, and chemotherapies present in the tumor microenvironment (TME) are capable of inducing EMT, but the role of the extracellular matrix (ECM) in this process remains poorly understood. Here, a novel tessellated three-dimensional (3D) polymer scaffolding is used to produce a fibrillar fibronectin matrix that induces an EMT-like event that includes phosphorylation of STAT3 and requires expression of β1 integrin. Consistent with these findings, analysis of the METABRIC dataset strongly links high-level fibronectin (FN) expression to decreased patient survival. In contrast, in vitro analysis of the MCF-10A progression series indicated that intracellular FN expression was associated with nonmetastatic cells. Therefore, differential bioluminescent imaging was used to track the metastasis of isogenic epithelial and mesenchymal cells within heterogeneous tumors. Interestingly, mesenchymal tumor cells do not produce a FN matrix and cannot complete the metastatic process, even when grown within a tumor containing epithelial cells. However, mesenchymal tumor cells form FN-containing cellular fibrils capable of supporting the growth and migration of metastatic-competent tumor cells. Importantly, depletion of FN allows mesenchymal tumor cells to regain epithelial characteristics and initiate in vivo tumor growth within a metastatic microenvironment.
Implications: In contrast to the tumor-promoting functions of fibronectin within the ECM, these data suggest that autocrine fibronectin production inhibits the metastatic potential of mesenchymal tumor cells. Mol Cancer Res; 16(10); 1579–89. ©2018 AACR.
The ability of epithelial cells to transition into a more primitive, migratory phenotype is an important process that occurs during wound healing and development. However, this capacity of epithelial cells to transition between these different phenotypes also supports the metastatic progression of breast cancer. Numerous model systems suggest that cells undergo a transient epithelial–mesenchymal transition (EMT) during invasion and dissemination, and then reverse that process through mesenchymal–epithelial transition (MET) during the outgrowth of secondary metastatic tumors (1–4). The importance of a highly plastic cell type to overcome the various stresses of the metastatic process is intuitively logical. However, the onset and reversal of EMT have also been linked to increased tumor-initiating capacity (5, 6). These studies raise exciting possibilities that EMT:MET may reactivate a fundamental genetic program capable of producing cells with an enhanced potential for adaptation to metastatic microenvironments and initiation of secondary tumors. Concurrent with these single-cell autonomous notions of EMT:MET and stemness is a growing concept supporting the importance of EMT-induced tumor cell heterogeneity (7). Heterogeneity within the stromal compartment of tumors is clearly important to metastasis as several critical paracrine signaling axes consisting of growth factors, hormones and adipokines have been described (8–10). However, numerous inducers of EMT can result in subpopulations of tumor cells with unique mechanical and molecular signatures that fall along a spectrum of epithelial to mesenchymal phenotypes (11, 12). Recent evidence suggests that more potent inducers of EMT can push epithelial tumor cells into a highly mesenchymal, stromal-like state and these cells have a reduced ability to undergo MET (13). What the drivers of these more stable mesenchymal phenotypes are, and how and if these stromal-like tumor cells continue to contribute to the metastatic process remains to be established.
In healthy tissues, stromal cells maintain the composition and structure of the tissue through production of extracellular matrix (ECM) proteins and paracrine signaling with epithelial cells (14). Both compositional and structural changes in the ECM have been observed during metastasis (15). One such ECM protein that can be produced by tumor cells following EMT is fibronectin (FN). Overall, increased FN expression in primary mammary tumors is strongly associated with decreased patient survival (16). Herein, we utilize a novel 3D culture system consisting of a tessellated scaffold to demonstrate that fibrillar FN can drive an EMT-like morphologic change, which allows for migration and proliferation of metastatic breast cancer cells independent of a hydrogel or polymer support. Counterintuitively, we find that breast cancer cells that constitutively express FN display an extremely stable mesenchymal phenotype and are not capable of completing metastasis. Therefore, we sought to address the hypothesis that autocrine production of FN by tumor cells limits their metastatic potential. Along these lines, genetic depletion of FN, but not its cognate receptor β1 integrin, allows tumor cells to regain epithelial characteristics and initiate tumor formation in the lungs.
Overall, our studies shed new light on the role of autocrine FN signaling during tumor growth and metastasis. Furthermore, we introduce a robust and versatile 3D cell culture approach capable of accurately recapitulating tumor microenvironment conditions that allow for controlled studies that cannot be accomplished in vivo or with other systems.
Materials and Methods
Ca1a and Ca1h cells were kindly provided by Dr. Fred Miller (Wayne State University, Detroit, MI). These cells were cultured in DMEM containing 10% FBS and penicillin/streptomycin. Stable expression of the luciferase, eGFP, or dTomato was achieved through lentiviral transduction and selection in puromycin or zeocin. For eGFP and dTomato expression, cells were sorted to increase uniform fluorescence across the entire population (Supplementary Fig. S1). Manipulation of FN expression was achieved through lentiviral-mediated transduction of TRCN0000064830, TRCN0000064832, a scrambled control shRNA (GE Dharmacon), or pLV (VectorBuilder) encoding full-length human FN or GFP as a control. In all cases, stable genomic integration of constructs was selected for using puromycin. HMLE cells were kindly provided by Sendurai Mani (MD Anderson Cancer Center, Houston, TX). These cells were cultured as described previously (16). Primary human pulmonary fibroblasts were obtained from ATCC and cultured in the recommended fibroblast basal media supplemented with fibroblast growth factor low serum kit (ATCC). Cells were validated for lack of contamination using IDEXX Impact III testing in April 2, 2014 and cryogenically frozen. All cell lines were used within one month of thawing.
All in vivo assays were conducted under institutional Animal Care and Use Committee approval from Purdue University (West Lafayette, IN). Where indicated, control or luciferase expressing Ca1a and Ca1h cells (2 × 106/50 μL) were injected into the second mammary fat pad of female 5-week-old, nu/nu mice. Thirty-five days after engraftment, tumors were surgically excised and metastasis was subsequently quantified by bioluminescent imaging. In other experiments, control and FN-depleted Ca1h cells (5×105 / 100 μL) were injected into the lateral tail vein of female 4-month-old, NSG mice. Pulmonary tumor growth was quantified by bioluminescence at the indicated time points. On the basis of previously established variability for bioluminescent imaging, 5 mice per group was chosen to adequately power our experiments to 0.80, with an α of 0.05.
For immunoblot analyses, cells were lysed using a modified RIPA lysis buffer containing 50 mmol/L Tris, 150 mmol/L NaCl, 0.25% sodium deoxycholate, 1.0% NP40, 0.1% SDS, protease inhibitor cocktail, 10 mmol/L activated sodium orthovanadate, 40 mmol/L β-glycerolphosphate and 20 mmol/L sodium fluoride. These lysates were separated by reducing SDS-PAGE and probed for β1 integrin, FGFR1 (Cell Signaling Technology), fibronectin, epithelial cadherin (Ecad), vimentin (BD Biosciences), zeb1, actin (Santa Cruz Biotechnology), zo-1 (Thermo Fisher Scientific), Ncad (R&D Systems), or β-tubulin (DSHB). For immunofluorescence, cells were fixed in 4% paraformaldehyde (PFA), permeablized in 0.1% Triton-X 100, and processed using fluorescently labeled phalloidin (Thermo Fisher Scientific) for visualization of the actin cytoskeleton, Ecad (BD Biosciences), or FN (Abcam). Where indicated, cellular monolayers were removed through incubation with 0.4% Triton, 1.5 NaCl, 50 mmol/L, Tris pH 8, and 50 mmol/L EDTA for 48 hours in 4°C, washed with water, incubated with 0.5% sodium deoxycholate at 25°C, and finally incubated with PBS (+Mgcl2) for 1 hour. Secreted proteins were precipitated from serum-free media by incubating 6 volumes of sample with 1 volume of 50% trichloroacetic acid and 1 volume of 0.1% sodium deoxycholate on ice for 30 minutes. Protein was precipitated via centrifugation and the pellet was twice washed with acetone and finally boiled at 95°C with 500 μL of 4× Laemmlli buffer. For flow cytometry, cells were fixed in 1% PFA, blocked in 2.0% BSA, and stained with antibodies against CD24 and CD44 (BioLegend) that were directly conjugated to the fluorescent probes. Patient samples stained for FN (DakoCytomation) by IHC were obtained from the protein atlas (17, 18). IHC analyses of formalin-fixed, paraffin-embedded tissue sections from Ca1h pulmonary tumors were conducted by deparafinization in xylene, rehydration, and antigen retrieval using 10 mmol/L sodium citrate (pH 6.0) under pressurized boiling. After inactivation of endogenous peroxidases in 3% H2O2, primary antibodies specific for Ecad (BD Biosciences), human vimentin (BD Biosciences), or Ki-67 (BD Biosciences), or FN (BD Biosciences) were added to serial sections and incubated overnight. Protein-specific staining was detected through the use of appropriate biotinylated secondary antibodies in conjunction with ABC reagent (Vector Laboratories). These sections were counterstained with hematoxylin, dehydrated, and mounted.
3D hydrogel assays
Fluorescent and bioluminescent Ca1a cells were mixed with nonlabeled or fluorescent Ca1a, Ca1h control, and Ca1h cells depleted in FN in 1:1 ratios and grown under 3D culture conditions. Cell growth was quantified via addition of luciferin (GoldBio). Briefly, 2,000 cells were plated in each well of a white-walled 96-well dish on top of a solidified 50 μL bed of Cultrex basement membrane extract (BME) from Trevigen. These cells were suspended in growth media containing DMEM, 10% FBS and 5% of the BME. For confocal microscopy, differentially labeled cells were grown under 3D culture conditions using 50-mm dish (MatTek) and images were taken using Zeiss 40× water dipping objective lens.
Production of 3D scaffolds
Scaffolds were produced using a photolithography-based approach, using the negative photo resist SU-8 2050 (Microchem). Silicon wafers were cleaned using a Plasma Tech RIE plasma cleaner, and dehydrated by baking at 120°C for 5 minutes. Omnicoat (Microchem) was used as a sacrificial layer. Three layers of Omnicoat were applied for each wafer using a spin coater at a spread speed of 500 rpm for 5 seconds, followed by 30 seconds at 1,000 rpm. After each layer was applied, the wafer was baked at 200°C for 1 minute, and then allowed to cool to room temperature. The SU-8 was then coated onto the wafer using a spread speed of 500 rpm for 5 seconds, followed by 1,700 rpm for 30 seconds. A final thickness of approximately 100 μm was attained. The wafer was then allowed to degass overnight at room temperature. After degassing, the wafers were baked at 65°C for 10 minutes, and then the temperature was increased to 95°C for an additional 50-minute bake. The wafers were then exposed to UV light using an Suss MA-6 mask aligner in hard contact mode, with a 20-second exposure time. A photomask was used to create the desired geometric pattern. After exposure, the wafer was baked for 5 minutes at 65°C followed by 10 minutes at 95°C. After cooling to room temperature, the wafers were developed in SU-8 developer for 11 minutes, rinsed in isopropanol (IPA), and then dried using compressed nitrogen gas. The developed scaffolds were then hard baked for 15 minutes at 150°C, and then released from the wafer using fresh SU-8 developer. The scaffolds were subsequently washed 6 times in IPA and allowed to dry overnight before use.
FN coating of scaffolds
Scaffolds were coated with FN by first mounting the scaffolds to a ferrous magnetic stainless steel frame using a cyanoacrylate-based adhesive. The mounted scaffolds were then placed in a 100 μg/mL solution of fibronectin, and then magnetically suspended at the air–water interface. The scaffolds were rotated for 2 hours on a rotisserie shaker that was maintained at 30°C with a rate of rotation of 8 rpm.
3D scaffold assays
Uncoated or FN-coated 3D scaffolds were placed in ultra low attachment 24-well dishes. Cells (50,000) were added to the scaffolds for 24 hours at which point nonadherent cells were washed away. For immunofluorescence, at day 6, the scaffolds containing the cells were fixed and stained with the indicated antibodies using protocols described above. Images were taken using a Zeiss 40× water dipping objective lens.
RNA was isolated using an RNA isolation kit (Omega Bio-tek). Total RNA was reverse-transcribed using a cDNA synthesis kit from (Thermo Fisher Scientific) and semi-quantitative real-time PCR was performed using iQ SYBR Green (Thermo Fisher Scientific). The following primers were used for the analysis. FN1 sense; ACAAACACTAATGTTAATTGCCCA, FN1 antisense; CCTCCAGAGCAAAGGGCTTA, CDH1 sense; GTTCAGACTCCAGCCCGC, CDH1 antisense; AAATTCACTCTGCCCAGGACG, VIM sense; CGGGAGAAATTGCAGGAGGA, VIM antisense; AAGGTCAAGACGTGCCAGAG
Two-way ANOVA or two-sided t tests were used where the data met the assumptions of these tests and the variance was similar between the two groups being compared. P values of less than 0.05 were considered significant. No exclusion criteria were utilized in these studies.
FN expression is associated with decreased patient survival
We have previously demonstrated an association between FN expression and decreased patient survival (16). Here, we analyzed the recent Molecular Taxonomy of Breast Cancer International Consortium (METABRIC) dataset consisting of more than 2,000 patient tumor biopsies (19). Significant outliers were observed in every subtype, with the claudin-low subtype having the outliers with the highest overall expression (Fig. 1A). When the dataset is taken as a whole, those patients above the mean or median expression level of FN demonstrated decreased survival compared with those patients below the mean or median (Fig. 1B and not shown). Finally, when separated into quartiles, those patients with the highest levels of FN demonstrate the shortest survival time (Fig. 1C). Overall, these data clearly indicate that high-level expression of the FN in primary tumors is strongly associated with decreased patient survival.
Nonmetastatic mesenchymal tumor cells aid the metastasis of responder cells within heterogeneous tumors
The MCF10CA1a (Ca1a) and the MCF10CA1h (Ca1h) cells are variants derived from the RAS-transformed MCF-10AT cells (20, 21). In culture, whole-cell lysates obtained from Ca1h cells demonstrate constitutive expression of FN and low levels of the epithelial marker, Ecad (Fig. 2A). In contrast, Ca1a cells fail to express detectable levels of FN but express robust amounts of Ecad (Fig. 2A). Somewhat counter to the patient data presented in Fig. 1, the FN-expressing Ca1h cells are considered to be invasive, but not metastatic, while the Ca1a cells are considered to be fully metastatic (21). However, it is difficult to directly compare the differential metastatic potential of the Ca1h and Ca1a cells in vivo due to drastic differences in primary tumor growth rates (Ca1h = 65.0 mg ± 17.32 mg; Ca1a = 983.4 mg ± 264 mg, 35 days post mammary fat pad engraftment of 2 × 106 cells). Furthermore, the metastatic rate of Ca1a primary tumors is very low, making inhibition of this process statistically challenging (Fig. 2B and C). Therefore, we sought to create mosaic tumors containing both Ca1h and Ca1a cells and track the metastasis of each cell type independently through differential labeling with firefly luciferase. Using this approach, 1:1 mixtures of Ca1a and Ca1h cells were orthotopically engrafted onto the mammary fat pad of nu/nu mice and these mosaic tumors were grown for 35 days (Fig. 2B). The primary tumors were surgically resected and the subsequent metastasis of each cell type was tracked by firefly bioluminescence (Fig. 2B and C). This approach indicated that even in a heterogeneous primary tumor, the Ca1a cells are clearly the cell type that forms metastatic lesions (Fig. 2B and C; Supplementary Fig. S2). These studies also revealed a highly significant increase in the metastatic efficiency of the Ca1a cells when grown in a mosaic tumor with the highly mesenchymal Ca1h cells (Fig. 2B and C). These data clearly indicate that while not competent for metastasis themselves, constitutively mesenchymal tumor cells can facilitate the metastasis of responder tumor cells in a paracrine manner.
Functionalized FN fibrils facilitate transient EMT and directional cellular migration
Previous studies suggest that FN contributes to metastasis through the induction of EMT (22, 23). To further characterize the role of FN in facilitating the heterotypic interactions between Ca1a and Ca1h cells, we initially attempted to use the Ca1h cells to create extracellular protein matrixes. However, consistent with previous studies, we observed that unlike fibroblasts, Ca1h cells do not deposit FN into a matrix (Fig. 3A and B; ref. 24). Therefore, we used a static adsorption coating method to coat tissue culture polystyrene (PS) with exogenous FN. Using this approach, we did observe increased cellular adhesion that was dependent on β1 integrin, a critical component of the FN receptor (Supplementary Fig. S3A and S3B). Consistent with previous reports, culturing the Ca1a cells on FN-coated PS did result in detectable modulation of EMT markers at the mRNA level (Supplementary Fig. S3C). However, using this approach, we did not observe a morphologic change in the Ca1a cells and we did not observe detectable changes in Ecad protein levels in these cells even after six consecutive passages on FN-coated plates (Supplementary Fig. S3D and S3E).
To achieve the fibrillar confirmation of FN that largely exists in vivo, we engineered a tessellated scaffold with 500 μm2 square pores, made of SU-8, which are capable of supporting the growth of cells when placed in nonadherent culture wells (Fig. 4A; Supplementary Fig. S4; refs. 25, 26). In contrast to static adsorption to a growth surface, we were able to create fibrillar FN by utilizing a rotational method to coat our 3D cell culture scaffolds (Fig. 4B). Importantly, only these FN fibrils contained cryptic binding domains, indicating enhanced functionalization of the ECM protein (Fig. 4B). The FN fibrils crossed the open spaces of the tessellated scaffold creating a controlled microenvironment for culture of the Ca1a cells free of interference from the polymer scaffold (Fig. 5A). Consistent with our coating of 2D polystyrene, Ca1a cells that remained on the solid support of the FN-coated scaffold maintained cell–cell junctions (Fig. 5A). However, the Ca1a cells that grew off the scaffold within the unsupported FN fibrils underwent an EMT-like morphologic change, characterized by activation of the cytoskeleton, dissolution of adherens junctions, and detection of STAT3 phosphorylation (Fig. 5A–C; Supplementary Fig. S5). These effects of fibrillar FN required expression of β1 integrin in the Ca1a cells (Fig. 5A–C; Supplementary Fig. S5). We were able to use time lapse microscopy to capture Ca1a cells migrating and proliferating on these pure FN fibrils (Supplementary Video S1).
To quantify this small subpopulation of cells growing within the FN fibrils, off the support of the scaffold, we assessed changes in the CD44 and CD24 populations by flow cytometry. A small but distinct population of Ca1a cells isolated from the FN-coated scaffolds demonstrated a mesenchymal CD44hi/CD24lo phenotype as compared with those same cells harvested from 2D polystyrene (Fig. 5D). This affect was again dependent on the expression of the FN receptor, β1 integrin (Fig. 5D). Similar to the Ca1a cells, culture of immortalized human mammary epithelial (HMLE) cells on functionalized FN-coated scaffolds also resulted in the emergence of a CD44hi, mesenchymal population that could be readily visualized upon return to 2D culture (Supplementary Fig. S6; refs. 5, 27).
Autocrine expression of FN stabilizes a constitutive mesenchymal phenotype
In contrast, to the requirement of β1 integrin for cellular response to fibrillar FN, depletion of β1 integrin or pharmacologic inhibition of integrin:FAK signaling using cyclic peptides or small-molecule kinase inhibitors in the Ca1h cells did not result in a return of epithelial characteristics (Supplementary Fig. S7A and S8B). In fact, shRNA-mediated depletion of β1 integrin led to increased levels of intracellular FN and diminution in Ecad expression in the T1K cells, an isogenic counterpart of the Ca1h cells (Supplementary Fig. S7A). Therefore, we sought to investigate potential integrin-independent functions of FN in EMT and metastasis that may be working in an intracellular fashion. Confocal microscopy confirmed strong colocalization of intracellular FN with the actin cytoskeleton (Supplementary Fig. S8). Depletion of FN in the Ca1h cells using two independent shRNAs led to increased transcript levels of the epithelial marker Ecad and loss of the mesenchymal marker vimentin, the intensity of which was consistent with the efficiency of FN depletion (Fig. 6A). In addition, depletion of FN caused altered protein expression of several but not all makers of MET including Ecad, Vimentin, Zeb1, Zo1, FGFR1, and cell surface expression of CD44 and CD24 (Fig. 6B and C). Accompanying these phenotypic markers, depletion of FN also lead a robust morphologic change in the Ca1h cells, resulting in the reduction of filamentous actin and the formation of adherens junctions (Fig. 6D and E). Taken together, these data are consistent with the conclusion that autocrine FN functions in a β1 integrin–independent fashion to maintain a stable mesenchymal phenotype.
Tumor cells expressing FN act in a stromal capacity to support the growth of other tumor cells
We next sought to characterize the interaction between FN-producing, constitutively mesenchymal tumor cells and metastatic tumor cells. To this end, we differentially identified Ca1a and Ca1h cells via stable expression and FACS for d-Tomato and eGFP, respectively (Supplementary Fig. S1). These cells were then cultured in a 3D hydrogel basement membrane matrix to assess the growth of the Ca1a cells alone or when in a heterogeneous coculture with the Ca1h cells. Growth of the Ca1a cells alone results in cell dense, spherical 3D structures (Fig. 7A). However, coculture of the Ca1a cells with FN-expressing Ca1h cells resulted in a loss of the spherical morphology, heterogeneous cell interspersion, and enhanced invasion of the Ca1a cells into the surrounding matrix (Fig. 7B, top). In addition, even when cells grew in close physical proximity, they did not form interspersed structures and the spherical growth pattern of the Ca1a structures was maintained (Fig. 7B, middle and bottom). Measuring bioluminescence production from the firefly luciferase expressing Ca1a cells allowed us to quantify their increased growth when in the presence of Ca1h cells (Fig. 7C). Decreased formation of heterogeneous cell clusters prevented this stromal support upon FN depletion in the Ca1h cells (Fig. 7C and D). These data suggest that FN expression by tumor cells allows them to act in a stromal fashion to physically support the growth of metastatic tumor cells.
Autocrine FN inhibits pulmonary tumor outgrowth
To more specifically characterize the autocrine versus paracrine role of FN in tumor growth we cultured control and FN-depleted Ca1h cells on our 3D scaffolds lacking any exogenous matrix coating. Addition of the Ca1h cells to the 3D scaffolds led to the formation of cellular fibrils that crossed the open spaces of the culture scaffolds (Fig. 8A; Supplementary Video S2). In contrast, Ca1h cells depleted in FN expression grew more robustly than control cells (Fig. 8B). However, FN-depleted cells remained on the solid support of the scaffold in an epithelial fashion, generating very distinct cortical actin (Fig. 8A–C; Supplementary Video S3–S4). Using our differentially labeled Ca1a and Ca1h cells, we were able to capture time-lapse microscopy demonstrating the ability of the Ca1a cells to utilize Ca1h cellular fibrils to migrate away from the culture scaffold (Supplementary Videos S5–S7). These data clearly demonstrate the ability of mesenchymal tumor cells to produce FN-containing cellular fibrils that are capable of facilitating cellular migration of metastatic tumor cells.
The increased proliferation of FN-depleted cells suggested that autocrine FN actively inhibits the ability of tumor cells to grow in a 3D environment. Along these lines, FN is also constitutively expressed by the D2.OR cell model of systemic dormancy as compared with their isogeneic and fully metastatic, D2.A1, counterparts (Supplementary Fig. S9; ref. 24). Therefore, we conducted tail-vein injection experiments to assess the in vivo capacity of control and FN-depleted Ca1h cells to initiate tumor growth within a physiologically relevant site of metastasis. Injection of control Ca1h cells resulted in detectable, but asymptomatic maintenance of these cells in the lungs over a period of 7 weeks (Fig. 8D–F). In contrast, FN-depleted Ca1h cells were capable of forming numerous macroscopic tumors within the pulmonary microenvironment (Fig. 8D–F). The bioluminescent signal from mice bearing control Ca1h cells was histologically located to a few small lesions within the lung (Fig. 8F; Supplementary Fig. S10). Consistent with our in vitro data, these smaller lesions that did form contained intracellular FN, but also demonstrated readily detectable levels of Ecad (Fig. 8F). Finally, we were unable to achieve stable overexpress FN in the Ca1a cells to a level that was consistent with that of the Ca1h cells (Fig. 8G). Nonetheless, even this moderate level of autocrine FN expression in the Ca1a cells was sufficient to modulate EMT markers, induce cellular fibril formation, decrease cell growth, and inhibit pulmonary tumor formation upon tail injection (Fig. 8G–J). Taken together, these data suggest that when presented as a homogenous inoculum, highly mesenchymal cells can undergo MET in the pulmonary microenvironment and proceed to macroscopic pulmonary tumor formation. However, these events are clearly inhibited by autocrine expression of FN.
Patient data presented here and elsewhere clearly demonstrate that high-level expression of FN within primary breast tumors is associated with decreased patient survival (16, 28). These clinical data are somewhat counter to data from tumor cell lines in which constitutive expression of autocrine FN corresponds to a nonmetastatic phenotype. Our cell labeling data clearly demonstrate that FN produced by tumor cells that have undergone an EMT contributes to the invasion and metastasis of their epithelial counterparts. Furthermore, our genetic depletion and overexpression studies indicate that production of FN stabilizes a nonmetastatic mesenchymal phenotype in an integrin-independent manner. This study supports the concept of epithelial–mesenchymal heterogeneity (EMH). In this scenario, stably mesenchymal tumor cells lose their cell-autonomous capacity for metastasis, but still contribute to metastatic progression by taking on a stromal role within the tumor microenvironment.
Consistent with our previous studies, we demonstrate that β1 integrin is required for fibrillar FN to promote the phosphorylation of STAT3, a molecule that is known to participate in the induction of EMT (16, 29). However, our data also suggest that cellular binding to fibrillar FN physically distorts cell morphology promoting a more mechanically induced mesenchymal morphology. Further studies detailing how fibrillar FN alters cell morphology and how these events relate to more transcriptionally driven EMT events induced by drugs and cytokines are clearly warranted. In addition, our studies suggest the concept of intracrine FN signaling. Indeed, as opposed to its requirement for response to fibrillar FN, depletion of β1 integrin does not cause an epithelial reversion as we observe upon depletion of FN. In fact, depletion of β1 integrin increased the levels of intracellular FN and enhanced a mesenchymal phenotype. While depletion of β1 integrin can have pleiotropic effects on cells, these data are consistent with a mechanism by which integrins facilitate the secretion of FN, a process that remains poorly understood in epithelial-derived cells. In addition, our microscopy studies suggest that intracellular FN directly interacts with the actin cytoskeleton, but more nanoscale analyses of these interactions are required. This and other potential mechanisms of how intracrine FN signaling may influence cell morphology and the molecular mechanisms that sustain constitutive FN expression in epithelial-derived tumor cells are areas of current investigation in our laboratory.
In addition to furthering our biological understanding of FN function and ECM-induced morphologic changes, a major advance of this study is development and implementation of our tessellated cell culture device capable of accurately recapitulating cellular and matrix phenotypes observed in vivo. Overall, our culture system represents advanced engineering that is easy to use and inexpensive to produce. As shown, cells cultured on ECM-coated or uncoated scaffolds can be readily grown and analyzed by immunofluorescence, harvested for immunoblot or mRNA analyses, trypsinized for flow cytometry, or passaged for continuous culture. All of these procedures can be done using techniques that are completely analogous to those currently used for standard 2D cell culture. Therefore, while other 3D culture systems are cumbersome and/or cost prohibitive for ongoing culture of stock cells our platform is well suited for long-term maintenance of cultured cell lines or primary, patient-derived tumor tissues.
In conclusion, we observed single-cell migration, loss of junctional Ecad, phosphorylation of STAT3 and gain of CD44 in cells cultured on FN fibrils. However, our studies do not rule out the possibility of tumor cells remaining in a transcriptionally epithelial state while migrating on cellular or FN fibrils. What is clear is that growth, migration, and overall metastasis of epithelial–mesenchymal malleable tumor cells is enhanced when in the presence of constitutively mesenchymal, FN-expressing tumor cells. These combined concepts of epithelial–mesenchymal plasticity and heterogeneity are likely both at play during metastasis, and model-dependent reliance on one or the other likely explains discrepancies between studies as to whether or not EMT contributes to metastasis (27, 28, 30, 31).
Disclosure of Potential Conflicts of Interest
No potential conflicts of interest were disclosed.
Conception and design: A. Shinde, A. Alpsoy, L. Solorio, M.K. Wendt
Development of methodology: A. Shinde, A. Alpsoy, L. Solorio, M.K. Wendt
Acquisition of data (provided animals, acquired and managed patients, provided facilities, etc.): A. Shinde, S. Libring, A. Abdullah, J.A. Schaber, L. Solorio, M.K. Wendt
Analysis and interpretation of data (e.g., statistical analysis, biostatistics, computational analysis): A. Shinde, S. Libring, A. Abdullah, L. Solorio, M.K. Wendt
Writing, review, and/or revision of the manuscript: A. Shinde, S. Libring, A. Alpsoy, A. Abdullah, J.A. Schaber, L. Solorio, M.K. Wendt
Administrative, technical, or material support (i.e., reporting or organizing data, constructing databases): L. Solorio, M.K. Wendt
Study supervision: L. Solorio, M.K. Wendt
This research was supported in part by the American Cancer Society (RSG-CSM130259; to M. Wendt) and the NIH (R01CA207751; to M. Wendt) and R00CA198929 (to L. Solorio), and the Purdue Center for Cancer Research via an NCI Center Grant (P30CA023168). We kindly acknowledge the expertise of the personnel within the Purdue Center for Cancer Research Biological Evaluation Core. We also acknowledge the use of the facilities within the Bindley Bioscience Center, a core facility of the NIH-funded Indiana Clinical and Translational Sciences Institute.
The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked advertisement in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.