Better understanding of the biophysical and biochemical cues of the tumor extracellular matrix environment that influence metastasis may have important implications for new cancer therapeutics. Initial exploration into this question has used naturally derived protein matrices that suffer from variability, poor control over matrix biochemistry, and inability to modify the matrix biochemistry and mechanics. Here, we report the use of a synthetic polymer-based scaffold composed primarily of poly(ethylene glycol), or PEG, modified with bioactive peptides to study murine models of lung adenocarcinoma. In this study, we focus on matrix-derived influences on epithelial morphogenesis of a metastatic cell line (344SQ) that harbors mutations in Kras and p53 (trp53) and is prone to a microRNA-200 (miR-200)–dependent epithelial–mesenchymal transition (EMT) and metastasis. The modified PEG hydrogels feature biospecific cell adhesion and cell-mediated proteolytic degradation with independently adjustable matrix stiffness. 344SQ encapsulated in bioactive peptide-modified, matrix metalloproteinase–degradable PEG hydrogels formed lumenized epithelial spheres comparable to that seen with three-dimensional culture in Matrigel. Altering both matrix stiffness and the concentration of cell-adhesive ligand significantly influenced epithelial morphogenesis as manifest by differences in the extent of lumenization, in patterns of intrasphere apoptosis and proliferation, and in expression of epithelial polarity markers. Regardless of matrix composition, exposure to TGF-β induced a loss of epithelial morphologic features, shift in expression of EMT marker genes, and decrease in mir-200 levels consistent with EMT. Our findings help illuminate matrix-derived cues that influence epithelial morphogenesis and highlight the potential utility that this synthetic matrix-mimetic tool has for cancer biology. Cancer Res; 72(22); 6013–23. ©2012 AACR.
Primary tumor invasion and metastasis is the leading cause of death in cancer patients, and epithelial–mesenchymal transition (EMT) is one principle mechanism driving metastasis. EMT is characterized by loss of epithelial polarity and intercellular adhesions and acquisition of mesenchymal features and migratory potential that permit invasion of tumor cells and dispersion to distant sites (1). The critical aspects of the tumor extracellular matrix (ECM) that promote or inhibit EMT and metastasis have not been fully characterized and remain an area of active investigation with potential for new therapeutic targets.
Initial exploration toward this goal has primarily focused on matrices from naturally derived materials such as collagen or Matrigel. It has been shown that increased density and organization of collagen-based matrices promote tumor progression in vitro and in vivo (2–4), and increased collagen cross-linking leads to EMT and invasion (5). Stiffening of Matrigel and collagen matrices perturbs epithelial morphogenesis of the MCF10A mammary cell line and promotes an invasive phenotype through alteration of integrin clustering and regulation of Rho activity and the FAK-ERK pathway (6; 7). Investigators have also begun to examine mechanical influences in synthetic matrix systems, but work thus far has largely been restricted to 2-dimensional (2D) culture on polyacrylamide gels (8–10).
A new lung adenocarcinoma model cell line panel has been developed in part to probe for similar ECM-related influences on lung cancer invasion and metastasis. These tumor cell lines, derived from a murine model with a somatically activated KRasG12D allele and a germline p53R172HΔG allele that produce primary lung adenocarcinoma with widespread metastatic disease (11), display an expression signature similar to that of human tumors from non–small cell lung adenocarcinoma patients with poor prognosis (12). Metastatic cell lines from this model (e.g., 344SQ) transition from a mesenchymal to epithelial phenotype when encapsulated in Matrigel, forming highly polarized, lumenized spheres that undergo EMT upon TGF-β exposure because of repression of the microRNA (miR)-200 family (13). Repression of miR-200 is required for the cells to undergo EMT and metastasize in syngeneic animals and drives a coordinated set of proinvasive changes in the expression of cell surface proteins and ECM matrix proteins (14). In addition, in vivo interactions of the tumor cells with the surrounding microenvironment at the leading edge drives the Jagged2-dependent development of a metastatic subpopulation, clearly suggesting that lung cancer behavior and metastatic progression may be highly influenced by contextual cues from and interactions with the ECM (15).
While the ease of use and high bioactivity of naturally derived matrices such as Matrigel, collagen and fibrin have facilitated this work and that of the bulk of the field, these matrices suffer important disadvantages and limitations. Matrigel batch-to-batch variability makes comparisons between studies difficult, and even growth factor-reduced preparations suffer from a high degree of contamination from hundreds to thousands of growth factors presenting unknown and unknowable experimental confounders (16–18). Both Matrigel and collagen matrices exhibit weak mechanical strength (E = 0.1–10 kPa), limiting their relevance in the study of higher range elasticities that may be more typical of cancerous soft tissue (E = 1–100 kPa) or stiffer sites of common metastasis such as bone (E >> 100 kPa) and presenting handling difficulties with more involved experimental manipulations (19, 20). Further, they feature a critical flaw in that the adjustment of matrix mechanics almost always alters matrix biochemistry, presenting a significant confounder (20–23), particularly in studies that strive to parse out the relative importance of ECM ligand and stiffness influences.
Synthetic hydrogels composed of poly(ethylene glycol), or PEG, offer an alternative 3-dimensional (3D) culture environment that provides independent control over biophysical and biochemical cues. These materials are composed of bioinert polymer chains with defined chemical structure and end groups that enable cross-linking. In tissue engineering applications, they have been well characterized as biologically inspired ECM mimetics (18). PEG hydrogels are commonly formed through mild photoinitiated polymerization techniques that permit cell encapsulation with high viability, showing an advantage over other synthetic matrices such as polyacrylamide hydrogels, which incorporate a highly toxic monomer component that prevents translation to 3D (24).
Along with biocompatibility, PEG hydrogels offer easily tunable and well-controlled bioactivity. Given the high degree of hydrophilicity, neutrality, and mobility of PEG, these hydrogels are highly resistant to the protein adsorption that mediates cell attachment to most synthetic materials, allowing an unmodified hydrogel to act as a cell-noninteractive “blank slate” with any bioactivity only present through well-controlled experimental intervention. This tunability and their versatility in use with many different cell types have lead to their widespread use in tissue engineering applications (25–28). Importantly, because the system is modular and the mechanical component is distinct from the bioactive component, these matrices feature independently tunable mechanics and biochemistry with each factor available for testing of an independent biologic effect with high experimental control.
In this work, we used such a PEG-based hydrogel system to study lung adenocarcinoma cell lines from the KRasG12D/p53R172HΔG murine model, with focus on a representative metastatic cell line, 344SQ, and compared its behavior in PEG matrices to that previously observed in the Matrigel system (13). We fabricated PEG hydrogels with varying elasticity and adhesive ligand concentration and probed for matrix-derived differences in epithelial morphogenesis and miR-200 regulation in response to TGF-β. In doing so we show that the more experimentally controllable synthetic hydrogel system is a useful tool for the cancer biologist to examine matrix-derived influences on tumor development and metastasis and an important improvement over the standard of the field.
Materials and Methods
The 344SQ, 393P, and 344P cell lines were derived from KRasG12D/p53R172HΔG mice as previously described (11; 13). The 344SQ_429 cells are derived from 344SQ parental cells and contain a constitutive expression vector encoding the miR-200b_a_429 locus (13; 14). Cells and cell-laden hydrogels were cultured in a humidified atmosphere at 37°C and 5% CO2 in RPMI 1640 (Mediatech) with 10% FBS (Atlanta Biologicals), 10 μg/mL gentamicin, and 0.25 μg/mL amphotericin B (Invitrogen).
Synthesis and purification of PEG-RGDS and PEG-PQ-PEG
Synthesis of PEG-RGDS has been previously described (26). Briefly, monoacrylate-poly(ethylene glycol)-succinimidyl carboxymethyl (PEG-SCM; Laysan Bio) and Arg-Gly-Asp-Ser peptide (RGDS; American Peptide) were mixed in dimethyl sulfoxide (Cambridge Isotope Laboratories) with a small volume of N, N-Diisopropylethylamine (DIPEA; Sigma) at molar ratios 1:1.2 and 1:2 (PEG-SCM: RGDS or DIPEA, respectively). After overnight reaction, the solution was dialyzed. PEG-PQ-PEG was synthesized by reaction with matrix metalloproteinase (MMP)-sensitive peptide GGGPQGIWGQGK (PQ). The PQ peptide was synthesized via standard Fmoc chemistry on an APEX 396 solid phase peptide synthesizer (Aapptec), characterized with MALDI-TOF, and then conjugated to PEG-SCM following a similar procedure as PEG-RGDS, but with a 2.1:1 molar ratio PEG-SCM:PQ. Conjugation of products was confirmed using gel permeation chromatography (Varian).
Cell encapsulation in hydrogels
Polymer mixtures were prepared sterilely with PEG-PQ-PEG (“PEG-PQ”) and PEG-RGDS in 10 mmol/L HEPES buffered saline (pH 8.3) with 1.5% v/v triethanolamine (Fluka BioChemika), 3.5 μL/mL N-vinylpyrrolidone (Sigma) and 10 μmol/L eosin Y photoinitiator (Sigma). Unless otherwise noted, PEG-PQ was mixed at 10% (w/v) and PEG-RGDS added at 3.5 mmol/L. 344SQ cells were pelleted by centrifugation at 500 × g for 4 minutes and then resuspended in the polymer solution at 1,500 cell/μL.
To create a hydrogel base for easy handling, cover glass was treated to introduce surface methacrylate groups as previously described (29). Hydrogel disks were fabricated by sandwiching a 5-μL droplet of polymer solution containing cells between a glass slide and a methacrylated glass cover slip separated by 380-μm-thick spacers and immediately exposing to white light for 30 s (Fiber-Lite Series 180, 150 W halogen, Dolan Jenner), leading to hydrogel polymerization and covalent linkage to the methacrylated cover glass base. High cell viability was confirmed 24 h after encapsulation (Live/Dead Kit, Invitrogen).
For material compressive properties, acellular hydrogel disks were formed as above using 5%, 10%, or 15% (w/v) PEG-PQ solutions. For comparison, Matrigel samples were prepared as previously described using a chamber plate with removable walls (13). Dimensions were obtained using digital calipers before subjecting samples (n = 4 per formulation) to compressive testing using an Instron Model 3340 mounted with a 10 N load cell. Instron Series IX/s software was used for testing control and data acquisition as uniaxial compressive strain was applied at 0.5 mm/min. Force-elongation data was converted to stress-strain data with corrected cross-sectional area and plotted to derive the elastic modulus from the slope of the linear portion of the curve.
344SQ sphere lumenization and size
344SQ cells were encapsulated in hydrogels with varied PEG-PQ concentration [5%, 10%, or 15% (w/v)] and fixed 3.5 mmol/L PEG-RGDS or with fixed 5% PEG-PQ concentration and varied PEG-RGDS concentration (1, 3.5, or 7 mmol/L) to assess matrix-related influences on the size and degree of lumenization of cell spheres. Hydrogel samples (n = 5 per formulation) were imaged every 2 days on an Axiovert 135 inverted fluorescent microscope (Zeiss), and sphere diameter was measured using Image J (NIH). Lumenization was quantified blinded to grouping as the number of spheres exhibiting central clearing over total spheres. Both size and lumenization data were expressed as means for all spheres in a given hydrogel sample. Further, size data from spheres across all hydrogel samples of a particular formulation were pooled and organized into histograms to better visualize matrix-related variation in sphere organization.
Hydrogel-encapsulated cells were fixed in 3.7% paraformaldehyde (EMS), permeabilized with 0.25% Triton X-100 (Sigma) and blocked overnight with 5% donkey serum (Sigma). Samples were then incubated with the following primary antibodies overnight at 4°C: mouse anti-β-catenin (BD Biosciences), mouse anti-α6-integrin (Chemicon), rabbit anti-ZO-1 (Invitrogen), rabbit anticleaved caspase-3 (Cell Signaling), or goat anti-ki-67 (Santa Cruz). Following rinse in PBS + 0.01% Tween (Sigma), samples were incubated overnight with an Alexafluor 488 or 555 tagged donkey anti-rabbit, mouse, or goat secondary antibody (Invitrogen), and counterstained with a 2 μmol/L 4′, 6-diamidino-2-phenylindole (DAPI) solution. Samples were imaged using a Zeiss 5Live confocal microscope.
Response to TGF-β and quantitative RT-PCR analysis
To observe responses to TGF-β, hydrogel-encapsulated 344SQ cells were cultured for 12 days to allow the formation of lumenized spheres, and then 5 ng/mL TGF-β1 (Calbiochem) was added to culture media. TGF-β-supplemented media was changed every 2 days. Samples were imaged on an Axiovert 135 inverted fluorescent microscope (Zeiss). Zymography was conducted to analyze for changes in MMP expression following TGF-β exposure using a 10% gelatin precast Ready Gel (BioRad) as previously described (25).
For RNA analysis, 344SQ cells were encapsulated at 3,000 cells/μL in hydrogels with matrix formulations as above (n = 6) and cultured for 10 days, after which half of the samples were treated for 4 days with TGF-β1 with daily supplemented media changes. Hydrogels were then digested with proteinase K (15 mg/mL, Calbiochem) for 2 minutes at room temperature, and then placed on ice before total RNA extraction with Trizol (Invitrogen) per manufacturer's protocol. Q-PCR was conducted on a 7500 Fast Real-Time PCR System (Applied Biosystems). The analysis of the miR-200 family levels (miR-200a, 200b, and 200c) and the mRNA for CDH1, CDH2, VIM, CRB3, and ZEB1 were conducted using TaqMan MiR assays (Applied Biosystems) and the data expressed relative to same-sample controls for miR-16 or L32, respectively.
PEG hydrogel fabrication and biophysical characterization
Reaction of PEG-SCM with short, bioactive peptides–created pegylated peptides that were incorporated to render hydrogels bioactive (Fig. 1A). Cell adhesion was promoted through use of the fibronectin-derived RGDS peptide with incorporation of PEG-RGDS as a scaffold pendant group. To enable cell-mediated proteolytic degradation of the base hydrogel, the MMP-2 and -9–degradable PQ peptide (30; 31) was similarly reacted to create a PEG-PQ molecule wherein the peptide is flanked by 2 monoacrylated PEG chains. PEG-based hydrogels composed of polymer chains of similar size as PEG-PQ possess water content more than 90%, volumetric swelling ratios (Q) of 10 to 20, and cross-link densities (ρx) of 0.5 to 1.5 mol/L, with molecular weight between cross-links (Mc) and mesh size sufficiently large to permit free diffusion of most biomolecules (respectively, ∼1,000 g/mol and 50–100 Å; refs. 32; 33). The mechanics of the hydrogel network were determined to be dependent on the amount of incorporated PEG-PQ. A series of hydrogels with increasing PEG-PQ concentration was subjected to uniaxial compressive mechanical testing to determine the elastic moduli, a measure of material stiffness (Fig. 1B). Five percent, 10%, and 15% PEG-PQ matrices had compressive moduli of 21 ± 6, 42 ± 8, and 55 ± 11 kPa, respectively. To provide context with previous work, Matrigel samples were also tested and found to be much softer than these PEG formulations with a compressive modulus of approximately 2.5 kPa. Encapsulation of cells did not significantly change the difference in elastic moduli between hydrogels of different PEG-PQ concentrations (Supplementary Fig. S1).
3D culture in bioactive PEG hydrogels recapitulates epithelial morphogenesis seen in Matrigel
Parental 344SQ lung adenocarcinoma cells were encapsulated in PEG-based hydrogel matrices by mixing with cell-degradable PEG-PQ and cell-adhesive PEG-RGDS in buffer in the presence of the photoinitiator eosin Y (Fig. 1C). The mild cross-linking conditions enabled high cell viability and, over several days in culture, cells proliferated, and formed multicellular spheres. After 7 to 10 days in culture, the cell clusters in PEG hydrogels (10% PEG-PQ/3.5 mmol/L PEG-RGDS) showed central clearing and formation of a lumen surrounded by an organized layer of single cells reminiscent of the lung acinus, closely mirroring the morphology seen in Matrigel (Fig. 2A and B). Cells encapsulated in the PEG-based matrix formulation generally formed smaller spheres (∼40 μm) than those in Matrigel (∼80 μm) and took longer to lumenize (7–10 days vs. 6–8 days, not shown; refs. 13).
To assess the extent of epithelial morphogenesis, structures were stained for epithelial polarity markers: α6-integrin marking the basolateral surface and zonula occludens-1 (ZO-1) for apical tight junctions. Lumenized PEG-encapsulated spheres showed distinct separation of polarity markers demonstrating clear formation of basolateral-apical polarity in a staining pattern comparable to that seen for Matrigel-encapsulated structures (Fig. 2C and D) and suggesting a mesenchymal-to-epithelial transition (MET). To show the PEG system as a reliable 3D culture platform across cancer models, other adenocarcinoma lines previously studied in Matrigel were encapsulated and stained for epithelial polarity markers β-catenin (basolateral) and ZO-1 (Fig. 2E–G). Another metastatic cell line derived from a primary tumor of KRasG12D/p53R172HΔG mice (344P) and the 344SQ_429 transfectant that constitutively expresses the miR200b_a_429 locus both formed lumenized spheres with epithelial polarity (Fig. 2E and F), whereas cells from the metastasis-incompetent 393P cell line formed disorganized cell aggregates (Fig. 2G), all of which mimics their respective behavior in Matrigel (13).
Matrix stiffness influences epithelial morphogenesis
Having established that a PEG-based system was capable of recapitulating the key epithelialization behavior exhibited by 344SQ in 3D Matrigel culture, we sought to examine the influence of key matrix parameters on this behavior. First, the PEG-PQ concentration, which forms the bulk of the material, was varied at 5%, 10%, or 15% while maintaining the cell-adhesive PEG-RGDS at a fixed 3.5 mmol/L. Utilizing higher polymer concentrations increased cross-link density and decreased mesh size, producing a stiffer matrix. Multicellular spheres formed in all matrix formulations, but spheres showed important differences in morphology and epithelialization behavior (Fig. 3A–C), with larger spheres and a lower percentage of lumenized structures in the softer, 5% PEG-PQ matrices. Monitoring sphere diameter with time (Fig. 3D) revealed that structures underwent rapid growth in the first few days of culture regardless of matrix stiffness, but growth persisted through day 8 only in the softer matrix (21 kPa), yielding spheres that were significantly larger relative to the other formulations (∼80 μm in 21 kPa hydrogels vs. ∼35 μm in the other formulations). An inverse relationship was observed for sphere lumenization (Fig. 3E); whereas all matrices exhibited increasing lumenization throughout the culture period, fewer encapsulated spheres were lumenized in the 21 kPa matrix (35%) compared with the 42 kPa matrix (50%). It was also observed that spheres in the 21 kPa matrix tended to be more heterogeneous in size and morphology relative to the stiffer matrix formulations, as reflected in histograms of pooled size data showing greater variation in sphere diameter in the softer gel (Fig. 3F and G and Supplementary Fig. S2). Additional exploration of sphere size differences indicated that cells in spheres in 21 kPa matrices were slightly larger than those in 42 kPa matrices (cell area at maximum sphere cross-section, 87.5 ± 22.7 μm2 vs. 63.6 ± 13.7 μm2, not significant) and, more notably, the number of cells in 21 kPa matrix spheres was greater than that in 42 kPa matrix spheres (cell number at maximum sphere cross-section, 22 ± 4 vs. 8 ± 2, P < 0.05), both contributing to overall differences observed in sphere diameter. This size difference may also be reflective of a difference in epithelial organization; work in other systems suggests that a transition to larger, less uniform structures indicates loss of epithelialization (6).
Samples from spheres grown in the hydrogel matrices were stained for proliferation/apoptosis and polarity markers to more closely assess matrix stiffness-related influences in sphere development and epithelialization (Fig. 4). Ki-67 staining revealed diffuse proliferation throughout spheres encapsulated in soft matrices at day 4 (Fig. 4A), whereas spheres in stiffer matrices exhibited a more localized peripheral staining pattern (Fig. 4B). Proliferation persisted through day 6 in 21 kPa matrices (Fig. 4C), but decreased in stiffer matrices as spheres became more completely lumenized (Fig. 4D). These observations correlated with differences in apoptosis as spheres in softer matrices showed unlocalized caspase-3 activity (Fig. 4C), whereas spheres in stiffer matrices showed strong core caspase activity (Fig. 4D). Furthermore, at day 6 the epithelial markers β-catenin (basolateral) and ZO-1 (apical) remained disorganized in softer matrices (Fig. 4E), whereas spheres in stiffer matrices (Fig. 4F) showed peripheral nuclear alignment and polar organization, albeit incomplete as β-catenin persisted on the apical edge. By day 12, however, lumenized spheres were found in both soft (Fig. 4G) and stiff (Fig. 4H) matrices, with these spheres exhibiting a high degree of epithelial organization and clear segregation of polar markers.
Adhesive ligand concentration influences epithelial morphogenesis
We next evaluated cell adhesive ligand concentration in the absence of changes to matrix stiffness, encapsulating 344SQ in matrices with a fixed 5% PEG-PQ concentration (21 kPa) and PEG-RGDS at 1 mmol/L (Fig. 5A), 3.5 mmol/L (Fig. 5B), or 7 mmol/L (Fig. 5C). Although spheres initially grew rapidly in all matrices, average sphere diameters (Fig. 5D) in 7 mmol/L PEG-RGDS matrices increased to only around 60 μm through day 6, whereas spheres in matrices with lower concentrations of adhesive ligand grew more rapidly and persistently up to 80 to 90 μm in diameter. The percentages of spheres lumenizing (Fig. 5E) showed a strong relationship with adhesive ligand concentration; spheres rapidly and more completely lumenized in 7 mmol/L PEG-RGDS, whereas after 12 days in culture a very low percentage of spheres (15%) lumenized in the 1 mmol/L group. It was also observed that incorporation of high concentrations of adhesive ligand into matrices induced formation of a much more homogenous sphere population (Fig. 5F and G). Supporting our interpretation that these changes are ligand-dependent, incorporation of varying amounts of PEG-RGDS did not result in changes to hydrogel mechanical properties (1 mmol/L 18.5 ± 4.6 kPa vs. 7 mmol/L 19.2 ± 3.8 kPa, not significant).
To further assess the influence of adhesive ligand concentration on epithelial morphogenesis, spheres in 21 kPa matrices with either 1 or 7 mmol/L PEG-RGDS were stained for markers of proliferation, apoptosis, and epithelial polarity (Fig. 6). While proliferation was extensive at day 4 in matrices with low PEG-RGDS concentration (Fig. 6A), it exhibited no localization pattern, whereas matrices with high PEG-RGDS induced more complete epithelial development with structures already exhibiting proliferation at the sphere periphery and central caspase-3 activity (Fig. 6B). At day 6, both sphere proliferation and apoptosis activity was scattered and diffuse in 1 mmol/L PEG-RGDS matrices (Fig. 6C). Meanwhile, structures in 7 mmol/L matrices had already developed into well-lumenized spheres (Fig. 6D). These observed differences in sphere development led to changes in epithelial organization; spheres in 1 mmol/L PEG-RGDS matrices adopted irregular morphologies by day 6 with spotty and unorganized expression of the basolateral and apical markers, β-catenin and ZO-1, respectively (Fig. 6E), whereas spheres in 7 mmol/L hydrogels formed lumens and developed appropriate apical-basal polarity (Fig. 6F). Well-organized spheres with clearly segregated polar edges were widely prevalent by 12 days in 7 mmol/L PEG-RGDS matrices (Fig. 6H). Although some spheres did lumenize in matrices with low concentrations of adhesive ligand, polarity markers remained disordered and morphology irregular with nuclei failing to arrange neatly around a cleared central lumen (Fig. 6G).
TGF-β induces EMT-related morphologic and epigenetic changes
Consistent with their metastatic behavior in vivo, TGF-β has been shown to initiate EMT in well-organized structures of 344SQ cultured in Matrigel through downregulation of miR-200 family member expression, inducing hyperproliferation, lumen filling, and matrix invasion (13). Probing for similar changes in spheres encapsulated in a PEG-based matrix (Fig. 7), lumenized spheres were allowed to form in matrices composed of 5% PEG-PQ with 7 mmol/L PEG-RGDS (Fig. 7A) and then exposed to soluble TGF-β. After 1 day of exposure (Fig. 7B), spheres began to lose organization and lumen clarity with epithelial organization continuing to diminish through 4 days of exposure (Fig. 7C) at which point lumens were completely filled. After 4 days of exposure, 0% of spheres were lumenized, polar organization was lost, and cells exhibited random proliferative and apoptotic activity (Supplementary Fig. S3). However, TGF-β response was not accompanied by a detectable increase in MMP expression (Supplementary Fig. S4).
To examine EMT-related microRNAs that may drive this morphologic change, quantitative RT-PCR was conducted to measure the changes in miR-200 levels and EMT markers following TGF-β treatment of spheres in matrices with fixed PEG-RGDS and varied PEG-PQ (Fig. 7D–G) or matrices with fixed PEG-PQ and varied PEG-RGDS (Fig. 7H–K). Regardless of matrix composition, miR200b levels were elevated before TGF-β and fell after exposure, coincident with the morphologic changes observed and similar to that seen in Matrigel-encapsulated spheres. Levels of miR-200a and miR-200c followed a similar pattern of decreased expression (Supplementary Fig. S5), indicating widespread epigenetic changes following TGF-β as miR-200b and miR-200c are found at 2 different chromosomal loci. Similarly, in all matrices, expression of epithelial marker genes decreased (CDH1 and CRB3) as expression of mesenchymal marker genes increased (CDH2, VIM, and ZEB1) indicating EMT was extensive (Fig. 7E–G and I–K, Supplementary Fig. S6).
In this report, we studied the behavior of murine lung adenocarcinoma cell lines in a 3D synthetic PEG hydrogel system, specifically focusing on the behavior of a highly plastic, model-metastatic cell line, and the independent influences of matrix mechanics and biochemistry on its epithelial morphogenesis. Our system is a significant advancement over the naturally derived matrix materials widely used in the field because a synthetic system with independently tunable modular components is the only way to reliably study the effect of these factors on cultured cells. Further, because tumor ECM is so complex and cancer cell behavior so exquisitely sensitive to changes in surrounding matrix environment, a “blank slate” system, completely free of uncontrolled sources of bioactivity, is essential to the goal of parsing out the relative significance of particular ECM cues on metastasis to enable identification of the most effective targets for further study and therapeutic development.
We showed that a PEG-based system, with simple bioactivity incorporated through the use of cell-adhesive PEG-RGDS and enzyme-degradable PEG-PQ backbone, was able to induce MET in 344SQ cells to form lumenized, polarized spheres similar to that observed in Matrigel. This observation was important as it suggests that this distinctive behavior is not dependent on excess bioactivity from residual growth factors or the presence of highly bioactive ECM components such as laminin found in high concentrations in Matrigel, but is simply a result of the innate differentiation capacity of these cells in a 3D environment. This observation also established the PEG system as a reliable platform to study matrix-derived influences on cancer cell behavior, a starting point from which the matrix may be further modified to probe for influences on this morphogenesis or EMT.
Two such modifiable characteristics are matrix mechanics and adhesive ligand concentration, which we showed to be highly tunable in our PEG system. The matrices examined in this study ranged from 21 to 55 kPa, but the PEG system can be tailored for either softer or stiffer matrices by varying the PEG base concentration or using a PEG chain with a different number of monomer repeats and molecular weight (22; 34). While all of the hydrogels tested were stiffer than Matrigel-based matrices, all were capable of supporting 344SQ culture and lumenized structure formation, suggesting that the comparatively softer Matrigel environment is not required for epithelial morphogenesis. Any alteration in cell behavior related to this softer environment may be compensated by the excessive bioactivity of the ligand-rich Matrigel.
Comparing 21 and 42 kPa matrices with fixed adhesive ligand, we found that epithelial structures were more organized in stiffer matrices as reflected by the rate and extent of lumenization and differences in sphere development and polar organization. This result runs counter to much of the work in the field that suggests high matrix stiffness favors less tumor organization and enhanced progression (5–7). The disparity may simply highlight the unpredictability of natural matrix biochemistry. Despite best efforts to incorporate similar bioactivity or mechanics, other investigators have shown that the same cells behave differently when cultured on Matrigel or other materials including collagen (35), naturally derived materials such as small intestinal submucosa (36) and polyacrylamide (37), suggesting it is very difficult to control for bioactivity in natural matrices such as Matrigel.
Our work was also an effort to disentangle mechanics from bioactivity, a difficult task with natural matrices in which mechanics and ligand density often change concordantly. Discerning the independent contribution of these factors is important given that collagen density, organization, and cross-linking are thought to promote tumor progression (3–5). Indeed, when investigators have deployed synthetic systems with better control over biochemistry and biomechanics, first using 2D polyacrylamide gels, in some cases cancer cells actually adopt a more benign, differentiated state on the stiffer substrate tested or display peak tumorogenic activity in matrices of intermediate stiffness (38–40). A few reports have transitioned this effort into 3D, finding a diminished invasive phenotype in the stiffer formulation of a hyaluronic acid based gel and enhanced epithelialization in stiffer collagen gels cross-linked with bioinert PEG (21; 41). However, the 2D polyacrylamide studies may offer limited insight into the more physiologic behaviors seen in 3D environments. The 3D systems are also imperfect as, despite attempts to control ligand concentration (21) and use bioinert cross-linkers (41), both of the bulk matrix components used are still themselves bioactive, inevitably leading to biochemical changes with increased cross-linking and stiffening.
In addition, while the bulk of work in the field has been done using a collection of the same commonly studied breast cancer model lines, when other cell lines have been examined, the matrix stiffness-related behavior observed is often highly dependent on the identity of the cell line tested or the nature and extent of its malignant transformation (8; 38; 39; 42–44). The cell lines studied here may exhibit either a different response to matrix stiffness or a higher degree of rigidity independence than the commonly used breast lines (8). Further, because very little work in the field has been done using cell lines that specifically and reliably model human lung adenocarcinoma, our work may highlight unique influences of matrix stiffness on metastatic properties of lung adenocarcinoma.
We also observed a pro-organizational effect of adhesive ligand in experiments altering PEG-RGDS concentration at a fixed matrix stiffness. This result is interesting in the context of results from the bulk of the field showing that a higher ligand concentration, usually collagen, leads to more aggressive tumors (3; 5). This disparity suggests that the identity of ECM ligand and the integrins subsequently bound are crucial to understanding the effect of ECM biochemistry on tumor progression. While little work in this regard has been done with fibronectin, from which RGDS is derived, this point is driven home by the many studies showing that, in contrast to collagen, increased laminin concentration promotes epithelial morphogenesis (35; 37). The PEG system has a unique advantage in that specific peptide sequences or domains from these large ECM molecules may be incorporated with high control and examined for a specific effect whereas, in other matrices, incorporation of a whole molecule with its multiple integrin binding sites may make the system too convoluted, leaving some matrix-derived signaling and gene expression events intractable.
Finally, we observed a repression of miR-200 levels following TGF-β exposure and concomitant shift in EMT marker gene expression. First, this finding is significant as it shows an ability to harvest and collect RNA from a 3D synthetic system, a nontrivial challenge to overcome when transitioning from natural to synthetic matrices. Furthermore, these epigenetic and gene expression changes show that the PEG-encapsulated cells engage physiological regulators of EMT, and that PEG is a useful 3D platform with which to study transcriptional events in response to extracellular signals. Moving forward, because the unmodified PEG matrix is a completely bioinert material, this system will enable much more robust study of additional ECM ligands and biochemical cues that may promote EMT and metastasis. In this vein, future work may modify the PEG system with additional peptides to engage different integrins or incorporate covalently tethered matrix-derived or cell–cell contact proteins that are integral to EMT. In addition, future studies may seek to use patterning techniques already deployed in tissue engineering applications to study 3D spatial relationships between tumors and ECM influences in an entirely new area of investigation (29; 45).
Disclosure of Potential Conflicts of Interest
No potential conflicts of interest were disclosed.
Conception and design: B.J. Gill, D.L. Gibbons, J.E. Saik, Z.H. Rizvi, J.L. West
Development of methodology: B.J. Gill, D.L. Gibbons, J.E. Saik, Z.H. Rizvi, J.L. West
Acquisition of data (provided animals, acquired and managed patients, provided facilities, etc.): B.J. Gill, D.L. Gibbons, L.C. Roudsari, J.E. Saik, Z.H. Rizvi, J.D. Roybal, J.M. Kurie
Analysis and interpretation of data (e.g., statistical analysis, biostatistics, computational analysis): B.J. Gill, D.L. Gibbons, J.E. Saik, Z.H. Rizvi, J.D. Roybal, J.M. Kurie, J.L. West
Writing, review, and/or revision of the manuscript: B.J. Gill, D.L. Gibbons, J.L. West
Administrative, technical, or material support (i.e., reporting or organizing data, constructing databases): B.J. Gill, J.D. Roybal
Study supervision: D.L. Gibbons, J.L. West
NIH R01 CA157450 (J.M. Kurie and J.L. West). NIH Biotechnology Training Program, 5T32 GM008362-19 (B.J. Gill). J.M. Kurie is the Elza and Ina A. Shackelford Endowed Professor in Lung Cancer Research. D.L. Gibbons was supported by NCI K08 CA151651, an International Association for the Study of Lung Cancer Fellow Grant, and received financial support from the Division of Cancer Medicine Advanced Scholars Program (MD Anderson Cancer Center). J.D. Roybal was supported by a career development award from the UT Southwestern/MD Anderson Cancer Center Lung Specialized Program of Research Excellence (P50 CA70907). Z.H. Rizvi was supported by the HHMI-Medical Research Fellows Program.
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.
The authors would like to thank the members of the West, Kurie, and Gibbons laboratories for assistance and comments on the work.
Note: Supplementary data for this article are available at Cancer Research Online (http://cancerres.aacrjournals.org/).
- Received March 7, 2012.
- Revision received July 25, 2012.
- Accepted August 13, 2012.
- ©2012 American Association for Cancer Research.