Cancer cells have the ability to migrate from the primary (original) site to other places in the body. The extracellular matrix affects cancer cell migratory capacity and has been correlated with tissue-specific spreading patterns. However, how the matrix orchestrates these behaviors remains unclear. Here, we investigated how both higher collagen concentrations and TGF-β regulate the formation of H1299 cell (a non-small cell lung cancer cell line) spheroids within 3D collagen-based matrices and promote cancer cell invasive capacity. We show that at low collagen concentrations, tumor cells move individually and have moderate invasive capacity, whereas when the collagen concentration is increased, the formation of cell clusters is promoted. In addition, when the concentration of TGF-β in the microenvironment is lower, most of the clusters are aggregates of cancer cells with a spheroid-like morphology and poor migratory capacity. In contrast, higher concentrations of TGF-β induced the formation of clusters with a notably higher invasive capacity, resulting in clear strand-like collective cell migration. Our results show that the concentration of the extracellular matrix is a key regulator of the formation of tumor clusters that affects their development and growth. In addition, chemical factors create a microenvironment that promotes the transformation of idle tumor clusters into very active, invasive tumor structures. These results collectively demonstrate the relevant regulatory role of the mechano-chemical microenvironment in leading the preferential metastasis of tumor cells to specific tissues with high collagen concentrations and TFG-β activity.
The seed and soil theory1 was proposed in the late 19th century and has greatly influenced cancer research. Cancer cells represent the seed, and their interactions with the microenvironment representing the soil, and this relationship was proposed as the main scheme to explain the ability of cancer to spread from its primary location to metastasize in secondary tissues. This theory attempted to explain why cancer does not metastasize randomly and instead exhibits a tissue-specific spreading pattern (tropism) dependent on the type of cancer. Numerous previous studies have focused on the roles of different microenvironmental characteristics and how they affect tropism and cancer dissemination2,3,4,5,6, but their results have not explained why different cancers exhibit different modes of migration.
Within this field, the involvement of the extracellular matrix (ECM) as a predictive biomarker of metastasis has recently attracted interest. ECM components are known to play significant regulatory roles in primary tumors by, for example, triggering tumor cell behaviors and invasion7,8,9,10,11. In particular, the roles of ECM mechanics in the regulation of cancer cell migration12,13 and malignancy development14,15 have been extensively explored. However, much less research has been focused on factors that affect the second site of future metastasis. Cell-ECM interactions and physical forces are known to play roles in guiding metastasis16,17,18, but the links between matrix properties and metastasis risk have not been fully explored.
Once circulating tumor cells reach a host tissue, they must adapt to the new microenvironment in order to survive. Their surveillance and proliferation activities are influenced by cell-cell and cell-matrix interactions in the metastatic niche19,20. The mechanical properties of the new soil tissue will impact the metastatic behavior of the infiltrating cells. The ECM of the metastatic niche is not simply a passive receiver of circulating tumor cells, its properties, including its composition, stiffness and pore size, provide feedback that affects the behavior of tumor cells. The resulting cross-talk may contribute to whether metastatic colonization is sustained21.
Collagen type I (ColI) is the main component of the ECM, and it constitutes the scaffold of the tumor microenvironment. Hence, the amount of ColI in the host tissue appears to be the ECM-related factor that is most important to generating the biochemical forces that form a supportive niche22. Changes in collagen concentrations could play a significant role in promoting the survival and growth of distant metastases and may support some zone-specific tumor spread23. Furthermore, ColI matrices are abundantly embedded with growth factors and cytokines, such as transforming growth factor-β (TGF-β), which can be released and activated during secondary site tumor colonization.
Therefore, in this study, we aimed to deepen our understanding of the mechanobiological factors that regulate this process and explore how differences in ColI concentrations and TGF-β stimulation directly regulate the key steps involved in metastasis. Here, we recreated and analyzed the behaviors exhibited by metastatic single cells once they reached secondary tissues. We exposed the cells to different collagen concentrations and TGF-β levels to study how these factors and related bio-chemo-mechanical characteristics modulate tumor colonization and surveillance.
For this analysis, we developed a 3D collagen matrix and microfluidics-based cell cultures to quantify the plasticity of the migratory capacity of metastatic non-small cell lung cancer (NSCLC) cells (H1299 cells) and evaluate how cell behaviors depend on the collagen concentration and the presence of TGF-β. Previous studies have shown that 3D in vitro cancer models provide numerous advantages over 2D models in studies aimed at exploring cancer malignancy24,25,26. For example, the differential matrix density responses of cancer cell lines have been correlated with tissue tropism27. Therefore, we used a simple collagen 3D culture system model to recreate metastatic conditions, and this allowed us to use live-cell microscopy to easily analyze differences in cell migration patterns.
In particular, we found that the collagen concentration in the 3D matrix and the level of TGF-β activation regulated differentiated patterns of cell migration and affected whether cells underwent individual or collective migration. Our results support the notion that the mechano-chemo-biological characteristics of the host tissue play crucial roles in determining the invasive capacity of tumor cells during metastasis.
Higher collagen concentrations reduce cancer cell migration
In this study, we sought to mimic the first key steps of tumor cell colonization to explore how different ECM environments affect cancer cell extravasation. First, we tested whether the migration of metastatic NSCLC cells was affected by different collagen concentrations. NCl-H1299 cells were selected as the model for metastatic cells in this study.
Cells were seeded in hydrogels with different concentrations of ColI (2.5, 4 and 6 mg/mL). These collagen-based hydrogels were mechanically characterized in a previous study28. Here, we quantified their architecture (Table 1) and found that the stiffness, pore size and porosity of the in vitro collagen matrices were similar to the ranges found in various living tissues12,29,30.
After cell harvesting, the cells were tracked for 24–48 h. The mean (instantaneous) and effective (accounting for only the starting and final positions) speeds were calculated under the indicated conditions. As the collagen concentration increased, the speed of cell migration (both mean and effective) (Fig. 1A) and the diffusion coefficient (as a measure of migration persistence) decreased (Fig. 1B), as expected13,30. In fact, we found that there the significant differences observed in cell speed were dependent on the collagen concentration (see Supplementary Videos #1, #2, and #3). This finding was not surprising because collagen density affects the strength of the physical barrier that interferes with cell migration by trapping single metastatic NSCLC cells to prevent their dissemination through the matrix. This phenomenon is known as steric hindrance31. Hence, cells become strongly confined when they encounter barriers with higher collagen concentrations, which make migration more arduous, ultimately leading to shorter cell trajectories (Fig. 1C).
Increasing the collagen concentration enhances cluster formation
After 5 days in 3D cell culture, single H1299 cells were able to proliferate under all conditions. However, different matrix-dependent morphologies were observed (Fig. 2A). Multicellular clusters of cells spontaneously formed in higher collagen concentrations (4 mg/mL and 6 mg/mL) and showed a rounded morphology with multiple DAPI-stained nuclei, whereas in 2.5 mg/mL collagen matrices, spreading single cells were mainly observed. In fact, as shown in Fig. 1C, cells were more capable of dissemination through the 2.5 mg/mL matrix, resulting in the formation of fewer clusters.
In contrast, as the collagen content increased, cluster formation increased, the proportion of single cells markedly decreased. Significant differences in the number of growing clusters were observed among the conditions. As shown in Fig. 2B, when the average number of clusters per microdevice was determined, the results indicated that very few clusters formed in softer matrices (1.15/device), whereas up to 23.5 and 33 clusters/device were counted in the 4 mg/mL and 6 mg/mL collagen concentrations, respectively. In all cases, we defined multicellular clusters as cell aggregates with an area larger than 1000 μm2.
H1299 spheroid growth is dependent on collagen gel concentration
We measured individual cell areas at different collagen concentrations at 24 h after seeding. Cluster growth was then monitored over 5 days.
On the first day, individual cell areas were larger in cells grown in higher collagen concentrations (Fig. 2C), in agreement with previous findings showing that malignant epithelial cells tend to occupy larger surface areas when grown on stiffer matrices15,32.
Cell proliferation caused the average area of the tumor clusters to grow dramatically over time in the 4 mg/mL (from ~500 to ~3000 μm2) and 6 mg/mL (from ~1000 to ~3750 μm2) collagen matrices (Fig. 2D), whereas the cells grown in softer matrices (2.5 mg/mL) did not tend to form clusters or increase cluster size.
The proliferative ability of H1299 cells enables these cells to form viable monoclonal clusters that start with single cells. By harvesting GFP-transfected H1299 cells together with non-fluorescent H1299 cells, we show that two types of predominant cell clusters develop: fluorescent and non-fluorescent ones. The general lack of mixed clusters demonstrates the monoclonal character of the clusters and implies that each cluster formed from a single initial cell (Fig. 2E).
TGF-β promotes cluster motility and a stretched morphology
We further analyzed the impact of epithelial cell TGF-β on the migration of single cells and cluster formation. TGF-β plays a dual role in human cancer by acting as either a tumor suppressor or a promoter of tumor metastasis33 depending on a variety of factors, such as the state of the disease34 and matrix rigidity35. Once local metastases take hold, local production of TGF-β can profoundly affect the growth of these lesions. The release of TGF-β in the vicinity of a secondary tumor is correlated with metastatic colony expansion and tumor reinitiation36,37. We sought to determine how TGF-β affects tumor cell migration in cells grown in different collagen concentrations and for different incubation times.
The cells were initially pre-treated with TGF-β for 3 days in 24-well plates before they were harvested for the 3D model. Then, individual cell migration was tracked. During the first 48 h, some differences were observed between pre-activated and non-activated individual cells in both migration speed and persistence (Fig. 3A,B). TGF-β seemed to have an effect on individual cell migration and its functional response may change in relation to matrix rigidity35,38,39. In fact, a multivariate statistical analysis revealed a strong interaction between collagen concentration and the presence of TGF-β (Fig. Sup. 3). With the addition of TGF-β, mean cell speed significantly decreased (−23%) at lower collagen concentrations (2.5 mg/ml), but increased or remained the same in denser matrices (4 and 6 mg/ml respectively). Changes in persistence (effective speed) were even more pronounced, decreasing almost a 40% in 2.5 mg/ml concentrations and rising a 30% in 4 mg/ml gels. Persistence also increased modestly (about 5%) in denser collagens (6 mg/ml) but this effect was statistically non-significant (see Table 2). Treatment with TGF-β seemed to activate molecular pathways that diminish steric hindrance effects at higher collagen concentrations (Fig. 3A). Based on this previous result, we performed another approach to study this phenomenon of interaction between collagen concentration and TGF-β. In this case, cells were cultured in 3D collagen matrices, and TGF-β activation was induced after gel polymerization. After seven days in 3D cell culture with 2.5 mg/mL matrices, the cells treated with TGF-β showed a morphological response and appeared as individual cells with a more elongated phenotype than was observed in the non-activated samples, in agreement with previous studies40. At higher collagen concentrations (4 and 6 mg/mL), cluster growth was stimulated and macroscopic changes were observed.
We quantified the roundness of the clusters formed at these concentrations by measuring the eccentricity of their occupying areas. We arbitrary defined an eccentricity threshold of 0.8 to differentiate spheroids (<0.8) from strands (>0.8). After cells were incubated for seven days in non-activated 3D cell culture (controls), cell clusters had an overall round morphology. However, when activated with TGF-β, the strand morphology was strongly promoted, especially in the 4 mg/mL collagen matrices (Fig. 4A,B). This effect was associated with a global increase in eccentricity values, which rose from 0.45 to 0.87 in 4 mg/mL collagen and from 0.46 to 0.65 in 6 mg/mL collagen (Fig. 3C,D).
The percentage of cells with a strand morphology increased from 12.5% in the control 4 mg/mL matrices to 45.7% in the TGF-β-activated matrices. There were also significant variations in the 6 mg/mL matrices, in which the strand percentage rose from 5.8% to 24.3% (Fig. 4B). This result suggests that TGF-β signaling induces changes in cell behavior and enhances strand tumor dissemination, at least within this range of collagen concentrations. Indeed, a multivariate statistical analysis revealed that the formation of spheroids is significantly dependent on collagen concentrations (p = 0,0017), while TGF-β determines the evolution to strand-shape clusters (p = 0,0004). In fact, the interaction between collagen and TGF- β to explain the formation of strands, was strongly non-significant (p = 0,6454) (Fig. Sup 5). Hence, these results indicate that TGF-β signaling plays a critical role in regulating collective migratory plasticity41.
Collective migration: migration is faster and more directed in strands than in spheroids
Migration parameters (cell speed, cell displacement and number of branches) were quantified in TGF-β-activated 4 mg/mL collagen matrices. We used bright-field time-lapse microscopy to follow the invasion pattern for 24 h to analyze cancer progression. During this time, the shapes of the spheroids remained stable while developing few or no branches (Fig. 5A), indicating poor invasiveness. Irregular cluster growth shifted the spheroids’ center of gravity, producing wiggling but ineffective movement (see Supplementary Video #4).
Conversely, strand-like clusters were capable of actively migrating through the matrix. We observed these cells acted cooperativity to produce a speed that highly surpassed that observed in slower spheroid migration (Fig. 5C). In fact, the strand-like clusters continued to increase in size while simultaneously developing the capacity to efficiently disseminate through the matrix at an average speed of 0.11 µm/min, which was faster than the 0.029 µm/min observed in cell spheroids. In addition, strand movement was much more directional in strands than in spheroids, as reflected by their significantly different effective speeds (0.025 and 0.0025 µm/min, respectively) (Fig. 5B). This cell behavior was directly related to the number of protruding arms or branches that emerged from the clusters. These branches appeared to lead the cells, and they constantly explored the cluster’s surroundings and sometimes dragged the entire body of the cluster in a specific direction. This dragging, in turn, generated the observed elongated morphology and eventually produced a substantial displacement of the cluster’s center of gravity (see Supplementary Video #5). Therefore, strand-like clusters were more likely to advance in the principal direction, and this enhanced the invasive capacity of these tumor cells.
Strand formation implies an integral reorganization of cell actin structures
Time-lapse movies and F-actin staining revealed that the movement of clusters in dense collagen matrices evolved from expansive growth movements to migration as strands. This process began at the cluster’s periphery, from which cell protrusions extended, and after a certain degree of structure strengthening was accomplished, these cells eventually escaped from the spheroid into the collagen and then started to pull the cluster’s body along while guiding its movement (see Supplementary Video 6). This reshaped morphology was accompanied by an alteration in F-actin localization. As shown in Fig. 6, actin fibers are clearly visible in cells with a strand morphology, whereas those in spheroids seem to have a focalized distribution pattern in which actin was localized at the cell cluster periphery. In contrast, in EdU assays, there were no significant differences in proliferative rates between spheroids and strand clusters (Fig. Sup. 6), indicating that TGF-β did not affect cell division.
In multicellular cancer invasion, steric hindrance and microtracks with dimensions smaller than the cell diameter (Table 1) caused the cells to become deformed and to aggregate42,43. In the cultures activated by TGF-β, the leader cells were located at the invasive front and were characterized by an altered morphology, which might had led to the generation and enlargement of predefined microtracks, eliminating the need for cell followers to generate new tracks44. Therefore, the observed intense actin polymerization may have been necessary to achieve harmonized migration.
In the present study, we harvested a metastatic NSCLC cancer cell line in microfluidic devices and varied both the ColI concentration and the presence of TGF-β to explore how ECM conditions play a role in the dissemination of cancer cells and contribute to the first steps of tumor colonization. We established how the microenvironment can regulate the plasticity modes observed in cancer migration, during which cells evolve from single to collective migratory modes, and quantified the dynamic and morphological factors that differed between these modes of invasion. Our initial results supported the hypothesis that a metastatic genotype is not the only parameter that plays an important role in tumor dissemination in all “soils”45 and indicate that both the collagen concentration and amount of TGF-β are important modulators of this process.
In a previous study, H1299 cells were inoculated into athymic mice via an intracardiac route, and the authors observed that the frequency of metastasis was higher in bone than in soft tissue46. Collagen-rich interstitial matrix is known to decrease cell velocity and consequently tissue invasion. Therefore, the following questions have arisen: why is the colonization of tumor cells (including the H1299 cell line) correlated with tissues with high ECM density, such as bone47, which has an ECM more than 105 times more rigid than that found in other matrices in soft tissues36,48? What explains the link, which has been reported both in vivo and in vitro, between desmoplasia (the growth of fibrous or connective tissue) and a higher probability of colonization by tumor cells49,50,51?
Our research results indicate that cancer cells grown in enriched collagen matrices migrate more slowly and tend to spontaneously form cell clusters22 and suppress single cell invasion. In dense matrices, cluster formation is induced by the high grade of cell confinement via a phenomenon called cell jamming52. The aggregated cell clusters present in metastases play a significant role in metastatic cell surveillance by increasing metastatic propensity and colony formation because they are more resistant to apoptosis at distal metastatic sites53,54,55,56. Therefore, as observed in this study, cell aggregation and cluster stability are enhanced in denser matrices. There, they are likely to promote cell surveillance during the first steps of colonization, even though they are associated with low invasive ability because the cells remain confined in the matrix region. Furthermore, we propose that using this cancer-on-a-chip system to study the cell-cell junctions that govern this process may offer valuable information, and we intend to use this approach in our future works.
In this work, we attempted to investigate the effects of the cytokines located in these high-density matrices on migration. TGF-β is known to play a major role in orchestrating such processes, including osteoblast-osteoclast signaling in bone remodeling, osteoclastic bone resorption57 and the development of fibrosis58. In fact, it has been argued that tumor cells embedded in these dense tissues produce factors that favor the increased release of TGF-β5,36. Furthermore, inhibiting the TGF-β pathway reduced the formation of bone metastases in preclinical models, and TGF-β seems to be related to the appropriate activation and progression of disseminated tumors36,37,59,60. On the other hand, there are numerous works35,38,39 which highlight the importance of integrin-TGF-β crosstalk and the manner that this pathway interaction controls the switch in cellular response to TGF- β induced by matrix rigidity, as it was quantified in this manuscript.
We next treated the denser collagen matrices (i.e., 4 and 6 mg/mL) with TGF-β. This treatment promoted the development of strand morphologies after 7 days, especially in cells grown in 4 mg/mL collagen, as previously shown. TGF-β signaling is well-known to break the junctional protein localization at the tumor-stromal interface and affect actin cytoskeleton reorganization trough Smad signaling pathway. Some studies have revealed that in the presence of TGF- β, tumors maintain E-cadherin membrane localization in multicellular lobular tumor structures but cytoplasmic localization or potential degradation in peripheral cells, promoting a strand-like migration42,52,61,62. This Collective-strand migration offers an effective and more aggressive invasion mode for multicellular units, minimizes the energy costs to individual cells and allows groups of cells to invade further and coordinate their movements with other cells, among other properties2,63,64. In this context, we found that the collective cell migration observed in the strand-like clusters grown in 4 mg/mL collagen had higher velocities than were observed in individual cells, even when we accounted for their fastest speeds on softer matrices (0.092 µm/min). This value (0.11 µm/min), which closely approached the velocities observed in in vivo intravital imaging experiments16, indicates that TGF-β exerted a strong effect by causing cells to switch between a mode encompassing expansive growth with minimum movement to one defined by a strand migration state with high invasiveness. Additionally, mechanical forces exerted by tumor cluster on extracellular microenvironment are likely to play a pivotal role in this migration mode switch induced by TGF-β and need further investigation.
Hence, we show that overt tumor colonization can be recreated under these conditions in microfluidic devices. These results provide a new perspective on the mechanism by which tumor cells overcome steric hindrance in dense matrices. The increased invasiveness and higher survivability of cell clusters may play a role in high collagen-TGF-β matrix tropism. Moreover, future approaches should use a diversity in tumor cell lines so that this hypothesis can be generalized and to unravel the molecular basis of the crosstalk observed between TGF-β and collagen39. As a proof of concept, a highly metastatic breast cell line (MDA-MB-231), that produces bone metastases27, was also tested under conditions including a high collagen concentration (6 mg/mL) and treatment with TGF-β. We achieved results (see Fig. Sup. 7) very similar to those found in NSCLCs. Therefore, and although this hypothesis should be explored in future experiments performed using many more and varied tumor cell lines, our results support the assumptions that a high collagen concentration regulates cluster growth and that TGF-beta mediates their capacity for invasion.
In summary, the collagen concentration of biological fiber matrices represents a strong physical limitation on the capacity of cancer cells to migrate and proliferate, suggesting that collagen concentrations regulate the formation and growth of tumor spheroids in metastatic tumors. Thus, a combination including a high collagen concentration and an environment rich in TGF-β will promote the capacity of tumor cells to invade host tissues (Fig. 7).
Materials and Methods
Microdevices were used according to the methodology described by Shin et al.65. Therefore, soft lithography was used to develop positive SU8 240-µm relief patterns with the desired geometry on a silicon wafer (Stanford University). Polydimethylsiloxane (PDMS, Sylargd 184, Dow Corning GmbH) was mixed at a 10:1 weight ratio of base to curing agent. The mixed solution was poured into the SU8 master and then degassed to remove air bubbles. Once the solution was cured, the replica-molded layer was trimmed, perforated and autoclaved. In the final step, the PDMS device and 35-mm glass-bottom petri dishes (Ibidi) were plasma-bonded and treated with poly-D-lysine (PDL) at 1 mg ml−1 (Sigma-Aldrich) with the aim of improving surface-matrix attachment.
The device geometry was based on that used by Farahat et al.66, which contained a central cage into which the hydrogel containing the embedded cells was deposited. In connection with the gel, it also had two side media channels that ensured hydration and the transport of nutrients and other chemical factors throughout the hydrogel (Fig. 8).
Hydrogel preparation and cell seeding
Metastatic NSCLC H1299 is a cell line that was derived from a metastatic site and expresses a variety of metastasis-promoting factors. H1299 cells were cultured using RPMI-1640 (Lonza) medium supplemented with 10% fetal calf serum (FCS, Life technologies). Cells were passaged or used for experiments when they reached 80% of confluence. H1299 cells were seeded into collagen-based hydrogels after sequential trypsinization and centrifugation. Finally, the cells were mixed with gel solutions at a final concentration of 0.2 × 106 cells/mL and pipetted into the gel cavities of the microdevice.
We followed the protocol described by Shin et al.65 Briefly, ColI (BD bioscience) was buffered to a final concentration of 2 mg/mL, 4 mg/mL, or 6 mg/mL with 10x DPBS containing calcium and magnesium (Thermo Fisher), cell culture-grade water (Lonza), and a previously prepared cell solution. The dilution was brought to pH 7.4 with NaOH.
Gel scaffold regions were filled with gel solution samples using auxiliary channels. The surface tension caused by the posts enabled the collagen gel solution to fix into the gel cavity. The gel-filled devices were then placed in prepared humid chambers in a CO2 incubator to allow the collagen to polymerize at 37 °C for 20 min. After polymerization, the gels were hydrated with RPMI and stored in the incubator for 24 h prior to conducting experiments. This incubation time ensured the stabilization of the matrix and cell adhesion and conditioning. The 3D systems were ready to use at 24 h after polymerization. The culture media (RPMI-1640, 10%FBS) was renewed in both media channels every day, and cells were cultured for 5–7 days.
Chemical activation: addition of TGF-ß
Different assays were performed to assess the effects of epithelial cell TGF-β (Miltenyi Biotec) on cancer cell migration (Fig. 9). The concentration of the recombinant human TGF-ß isoform employed in these experiments was 10 ng/ml67.
In one group (Fig. 9A), the cells were treated with 10 ng/ml of TGF-β for three days in 24-well cell culture plates and subsequently harvested and placed in 3D microdevices. In these experiments, individual cell migration was studied at 24 h after cell seeding.
In a second group (Fig. 9B), the cells were first seeded without previous TGF-β treatment. After the cells were embedded in 3D collagen matrices with different collagen concentrations, they were stimulated with TGF-β for seven days. The cell media containing TGF- β (10 ng/ml) was replaced once every day. Cell morphology and collective migration were subsequently evaluated after seven days.
Immunofluorescence staining and imaging
The samples were stained with DAPI and phalloidin and imaged using a Nikon D-Eclipse C1 confocal microscope equipped with a Plan Apo VC 60XH objective and an Olympus Fluoview FV10i confocal microscope equipped with an UPLSAPO 60XW objective. The cells were fixed in 4% paraformaldehyde (Affymetrix) in PBS for 20 min at room temperature, washed three times with PBS and permeabilized with 0.1% Triton X-100 (Calbiochem) in PBS. The cells were washed three washes more times and then blocked in 3% goat serum (Sigma) in 5% BSA/PBS solution for 4 h at room temperature. Afterwards, the devices were incubated overnight at 4 °C in the dark with Alexa Fluor® 594-phalloidin conjugates (A12381, Molecular Probes). Then, the samples were washed 3 times with 0.5% BSA/PBS, and the devices were incubated for 4 h at 4 °C in the dark with DAPI (Invitrogen). Finally, the cells were washed 3 more times and imaged.
To study cell proliferation in cell clusters and strands, the cells were cultured with 10 µl of EdU (Merck) per ml of culture medium for 24 h prior to imaging acquisition. The cells were fixed with paraformaldehyde and permeabilized with Triton X-100. The cells were incubated for 30 minutes with the following reaction cocktail for cell staining: 6-FAM Azide, Catalyst solution, and Reaction buffer (Merck).
Cell tracking and morphology quantification
Time-lapse imaging was carried out by acquiring phase-contrast images every 20 min for 24 h to study individual cell migration. The focal plane located in the middle of the device along the z-axis was selected, and out-of-focus cells were not quantified to minimize artifacts resulting from the glass and PDMS surfaces. This approach ensured that the tracked cells were fully embedded within the 3D network. The incubation conditions were controlled at 37 °C, 5% CO2 and 95% humidity. Approximately 50 cells in each set of experimental samples were tracked. Cell trajectory acquisition was performed using a hand-coded semi-automatic MATLAB script described in previous studies68,69,70. By comparing pixel intensities and using matrix convolution techniques, the software was able to find and track cell centroids, request visual correction from the user, and post-process the migration results. These trajectories were used to extract the cell mean (Vmean) and effective (Veff) velocities. Note that Vmean is defined as the averaged instantaneous speed including all time steps, whereas Veff takes into account only the initial and final positions. The MSD curve of each trajectory was also obtained and used to determine the global diffusion coefficient (D), which was used as a measure of migration persistence in a linear-weighted fit of the mean MSD curve (using the first quarter of the data). Additionally, MSD individual curves were used to fit a power law (MSD(t) = γ.tα)) to determine the kind of motion (α < 1 for confined motion, α = 1 for Brownian or purely diffusive motion and α > 1 for directed motion)71.
Cluster/strand morphological characteristics were also obtained with a MATLAB hand-coded script. We compared the roundness of formed clusters/strands in different experiments using eccentricity as a measurable scalar parameter that was defined as the ratio of the distance between the foci of the ellipse that fit the cluster/strand (the ellipse with the same second-moments as the region) to its major axis length. The values ranged between 0 and 1, with 0 indicating a circle and 1 indicating a line segment. The geometrical centroids of clusters/strands were tracked over time to extract their migration parameters.
Quantification of hydrogel porosity and pore size
DQ-Collagen™ type I from a bovine skin fluorescein conjugate (Thermo Fisher) (final concentration: 25 µg/ml) was added to 2.5, 4 and 6 mg/ml hydrogels to analyze the disposition of the collagen fibers inside the hydrogel72. The fluorescence of this reactant was used to analyze the architecture of the 2.5 and 4 mg/ml collagen hydrogels. Due to the high density of the 6 mg/ml collagen gels, the procedure used to visualize this hydrogel was performed using confocal reflectance to improve the quality of the images. A Zeiss LSM 880 confocal microscope equipped with a Plan Apochromat 1.4 63x/1.40 Oil objective was used to visualize the hydrogels.
Confocal cross-section images were sequentially acquired at one point at the center of each microdevice with a constant step size of 0.5 µm. The 3D reconstruction of the z-stack of images of the collagen network was carried out via 3D skeletonization using the FIRE algorithm73,74 to obtain a binary stack. From the 3D reconstruction, we quantified the porosity by dividing the total volume of pores between the total volume of the sample being analyzed. Furthermore, we calculated the pore size with another previously described method75. Briefly, pore size was determined by obtaining the distribution of the nearest obstacle distances (NODs, defined as the Euclidean distance from a point in the liquid phase to the nearest point in the solid phase).
Paget, S. The distribution of secondary growths in cancer of the breast. Lancet 133, 571–573 (1889).
Friedl, P. & Alexander, S. Cancer invasion and the microenvironment: Plasticity and reciprocity. Cell 147, 992–1009 (2011).
Brábek, J., Mierke, C. T., Rösel, D., Veselý, P. & Fabry, B. The role of the tissue microenvironment in the regulation of cancer cell motility and invasion. Cell Commun. Signal. 8, 22 (2010).
Peinado, H. et al. Pre-metastatic niches: organ-specific homes for metastases. Nat. Rev. Cancer (2017).
Obenauf, A. C. & Massagué, J. Surviving at a Distance: Organ-Specific Metastasis. Trends in Cancer 1, 76–91 (2015).
Kenny, P. A. et al. The morphologies of breast cancer cell lines in three-dimensional assays correlate with their profiles of gene expression. Mol. Oncol. 1, 84–96 (2007).
Seewaldt, V. ECM stiffness paves the way for tumor cells. Nat. Med. 20, 332–333 (2014).
Carey, S., Martin, K. & Reinhart-King, C. Three-dimensional collagen matrix induces a mechanosensitive invasive epithelial phenotype. Nat. Publ. Gr. 1–14 (2017).
Kopanska, K. S., Alcheikh, Y., Staneva, R., Vignjevic, D. & Betz, T. Tensile forces originating from cancer spheroids facilitate tumor invasion. PLoS One 11, 1–23 (2016).
Lu, P., Takai, K., Weaver, V. M. & Werb, Z. Extracellular matrix degradation and remodeling in development and disease. Cold Spring Harb Perspect Biol 3, 1–24 (2011).
William, J., Zervantonakis, I. K., Roger, D. & Link, C. Tumor cell migration in complex microenvironments. Cell Mol Life Sci 70, 1335–1356 (2015).
Doyle, A. D., Carvajal, N., Jin, A., Matsumoto, K. & Yamada, K. M. Local 3D matrix microenvironment regulates cell migration through spatiotemporal dynamics of contractility-dependent adhesions. Nat. Commun. 6, 8720 (2015).
Krause, M. & Wolf, K. Cancer cell migration in 3d tissue: Negotiating space by proteolysis and nuclear deformability. Cell Adhes. Migr. 9, 357–366 (2015).
Lachowski, D. et al. Substrate Rigidity Controls Activation and Durotaxis in Pancreatic Stellate Cells. Sci. Rep. 7, 2506 (2017).
Paszek, M. J. et al. Tensional homeostasis and the malignant phenotype. Cancer Cell 8, 241–254 (2005).
Gligorijevic, B., Bergman, A. & Condeelis, J. Multiparametric Classification Links Tumor Microenvironments with Tumor Cell Phenotype. PLoS Biol. 12 (2014).
Barney, L. E. et al. A cell–ECM screening method to predict breast cancer metastasis. Integr. Biol. 7, 198–212 (2015).
Barney, L. E. et al. The predictive link between matrix and metastasis. Curr. Opin. Chem. Eng. 11, 85–93 (2016).
Cox, T. R. et al. LOX-mediated collagen crosslinking is responsible for fibrosis- enhanced metastasis. Cancer Res 73, 1721–1732 (2013).
Massagué, J. & Obenauf, A. C. Metastatic colonization by circulating tumour cells. Nature 529, 298–306 (2016).
Harjanto, D., Maffei, J. S. & Zaman, M. H. Quantitative analysis of the effect of cancer invasiveness and collagen concentration on 3D matrix remodeling. PLoS One 6 (2011).
Sapudom, J. et al. The phenotype of cancer cell invasion controlled by fibril diameter and pore size of 3D collagen networks. Biomaterials 52, 367–375 (2015).
Multhaupt, H. A. B., Leitinger, B., Gullberg, D. & Couchman, J. R. Extracellular matrix component signaling in cancer. Adv. Drug Deliv. Rev. 97, 28–40 (2016).
Sun, W., Lim, C. T. & Kurniawan, N. A. Mechanistic adaptability of cancer cells strongly affects anti-migratory drug efficacy. J. R. Soc. Interface 11, 20140638–20140638 (2014).
Li, R. et al. Macrophage-secreted TNFα and TGFβ1 influence migration speed and persistence of cancer cells in 3D tissue culture via independent pathways. Cancer Res. 77, 279–290 (2017).
Jeong, S. Y., Lee, J. H., Shin, Y., Chung, S. & Kuh, H. J. Co-culture of tumor spheroids and fibroblasts in a collagen matrix-incorporated microfluidic chip mimics reciprocal activation in solid tumor microenvironment. PLoS One 11, 1–17 (2016).
Kostic, A., Lynch, C. D. & Sheetz, M. P. Differential matrix rigidity response in breast cancer cell lines correlates with the tissue tropism. PLoS One 4 (2009).
Valero, C. et al. Combined experimental and computational characterization of crosslinked collagen- based hydrogels. PLoS One. 13(4) (2018)
Buxboim, A., Ivanovska, I. L. & Discher, D. E. Matrix elasticity, cytoskeletal forces and physics of the nucleus: how deeply do cells ‘feel’ outside and in? J. Cell Sci. 123, 297–308 (2010).
Wolf, K. et al. Physical limits of cell migration: Control by ECM space and nuclear deformation and tuning by proteolysis and traction force. J. Cell Biol. 201, 1069–1084 (2013).
Lange, J. & Fabry, B. Cell and tissue mechanics in cell migration. Exp Cell Res 76, 211–220 (2012).
Butcher, D. T., Alliston, T. & Weaver, V. M. A tense situation: forcing tumour progression. Nat. Rev. Cancer 9, 108–22 (2009).
Lebrun, J.-J. The Dual Role of TGF -β in Human Cancer: From Tumor Suppression to Cancer Metastasis. ISRN Mol. Biol. 2012, 1–28 (2012).
Massagué, J. TGFβ in Cancer. Cell 134, 215–230 (2008).
Leight, J. L., Wozniak, M. A., Chen, S., Lynch, M. L. & Chen, C. S. Matrix rigidity regulates a switch between TGF- 1-induced apoptosis and epithelial-mesenchymal transition. Mol. Biol. Cell 23, 781–791 (2012).
Croucher, P. I., McDonald, M. M. & Martin, T. J. Bone metastasis: the importance of the neighbourhood. Nat. Rev. Cancer 16, 373–86 (2016).
Buijs, J. T., Stayrook, K. R. & Guise, T. A. The role of TGF-β in bone metastasis: novel therapeutic perspectives. Bonekey Rep. 1, 96 (2012).
Ruppender, N. S. et al. Matrix rigidity induces osteolytic gene expression of metastatic breast cancer cells. PLoS One 5, 1–10 (2010).
Margadant, C. & Sonnenberg, A. Integrin–TGF-β crosstalk in fibrosis, cancer and wound healing. EMBO Rep. 11, 97–105 (2010).
Shintani, Y., Maeda, M., Chaika, N., Johnson, K. R. & Wheelock, M. J. Collagen I promotes epithelial-to-mesenchymal transition in lung cancer cells via transforming growth factor-β signaling. Am. J. Respir. Cell Mol. Biol. 38, 95–104 (2008).
Matise, L. A. et al. Lack of transforming growth factor-β signaling promotes collective cancer cell invasion through tumor-stromal crosstalk. Breast Cancer Res. 14, R98 (2012).
Wu, J., Sheng, S., Liang, X. & Tang, Y. The role of tumor microenvironment in collective tumor cell invasion. Futur. Oncol. 13(11), 991–1002 (2017).
Ilina, O., Bakker, G.-J., Vasaturo, A., Hoffman, R. M. & Friedl, P. Two-photon laser-generated microtracks in 3D collagen lattices: principles of MMP-dependent and -independent collective cancer cell invasion. Phys. Biol. 8, 029501–029501 (2011).
Gaggioli, C. et al. Fibroblast-led collective invasion of carcinoma cells with differing roles for RhoGTPases in leading and following cells. Nat. Cell Biol. 9, 1392–1400 (2007).
Nguyen-Ngoc, K.-V. et al. ECM microenvironment regulates collective migration and local dissemination in normal and malignant mammary epithelium. Proc. Natl. Acad. Sci. 109, E2595–E2604 (2012).
Singla, A. K., Downey, C. M., Bebb, G. D. & Jirik, F. R. Characterization of a murine model of metastatic human non- small cell lung cancer and effect of CXCR4 inhibition on the growth of metastases. Oncoscience 2, 263–71 (2015).
Coleman, R. E. Skeletal complications of malignancy. Cancer 80, 1588–94 (1997).
Clarke, B. Normal bone anatomy and physiology. Clin. J. Am. Soc. Nephrol. 3, 131–139 (2008).
Cox, T. R. & Erler, J. T. Breast Cancer Management Fibrosis, cancer and the premetastatic niche. Breast Cancer Manag 3, 453–455 (2014).
Cox, T. R. & Erler, J. T. Fibrosis and Cancer: Partners in Crime or Opposing Forces? Trends in Cancer 2, 279–282 (2016).
Aiello, N. M. et al. Metastatic progression is associated with dynamic changes in the local microenvironment. Nat. Commun. 7, 12819 (2016).
Haeger, A., Krause, M., Wolf, K. & Friedl, P. Cell jamming: Collective invasion of mesenchymal tumor cells imposed by tissue confinement. Biochim. Biophys. Acta - Gen. Subj. 1840, 2386–2395 (2014).
Aceto, N. et al. Circulating tumor cell clusters are oligoclonal precursors of breast cancer metastasis. Cell 158, 1110–22 (2014).
Cheung, K. J. et al. Polyclonal breast cancer metastases arise from collective dissemination of keratin 14-expressing tumor cell clusters. Proc. Natl. Acad. Sci. 113, E854–E863 (2016).
Cheung, K. J. & Ewald, A. J. A collective route to metastasis: Seeding by tumor cell clusters. 352, 167–170 (2016).
Maddipati, R., Stanger, B. Z. & Division, G. Cancer Discov. 5(10), 1086–97 (2015).
Erlebacher, A., Filvaroff, E. H., Ye, J. Q. & Derynck, R. Osteoblastic Responses to TGF-β during Bone Remodeling. Mol. Biol. Cell 9, 1903–1918 (1998).
Cox, T. R. & Erler, J. T. Molecular pathways: Connecting fibrosis and solid tumor metastasis. Clin. Cancer Res. 20, 3637–3643 (2014).
Sterling, J. A., Edwards, J. R., Martin, T. J. & Mundy, G. R. Advances in the biology of bone metastasis: How the skeleton affects tumor behavior. Bone 48, 6–15 (2011).
Juárez, P. & Guise, T. A. TGF-B in cancer and bone: Implications for treatment of bone metastases. Bone 48, 23–29 (2011).
Kumar, S., Kapoor, A., Desai, S., Inamdar, M. M. & Sen, S. Proteolytic and non-proteolytic regulation of collective cell invasion: tuning by ECM density and organization. Nat. Publ. Gr. 1–17 (2016).
Gjorevski, N., Piotrowski, A. S., Varner, V. D. & Nelson, C. M. Dynamic tensile forces drive collective cell migration through three-dimensional extracellular matrices. Sci. Rep. 5, 11458 (2015).
Lintz, M., Muñoz, A. & Reinhart-King, C. A. The Mechanics of Single Cell and Collective Migration of Tumor Cells. J. Biomech. Eng. 139, 1–9 (2016).
Friedl, P. Prespecification and plasticity: Shifting mechanisms of cell migration. Curr. Opin. Cell Biol. 16, 14–23 (2004).
Shin, Y. et al. Microfluidic assay for simultaneous culture of multiple cell types on surfaces or within hydrogels. Nat Protoc. 7(7), 1247–1259 (2014).
Farahat, W. A. et al. Ensemble analysis of angiogenic growth in three-dimensional microfluidic cell cultures. PLoS One 7 (2012).
Wu, Y.-C., Tang, S.-J., Sun, G.-H. & Sun, K.-H. CXCR7 mediates TGFβ1-promoted EMT and tumor-initiating features in lung cancer. Oncogene 1–10 (2015).
Moreno-Arotzena, O., Mendoza, G., Cóndor, M., Rüberg, T. & García-Aznar, J. M. Inducing chemotactic and haptotatic cues in microfluidic devices for three-dimensional in vitro assays. Biomicrofluidics 8, 1–15 (2014).
Moreno-Arotzena, O., Borau, C., Movilla, N., Vicente-Manzanares, M. & García-Aznar, J. M. Fibroblast Migration in 3D is Controlled by Haptotaxis in a Non-muscle Myosin II-Dependent Manner. Ann. Biomed. Eng. 43, 3025–3039 (2015).
del Amo, C., Borau, C., Gutiérrez, R., Asín, J. & García-Aznar, J. M. Quantification of angiogenic sprouting under different growth factors in a microfluidic platform. J. Biomech (2016).
Tarantino, N. et al. Tnf and il-1 exhibit distinct ubiquitin requirements for inducing NEMO-IKK supramolecular structures. J. Cell Biol. 204, 231–245 (2014).
Hoshino, D. et al. Exosome secretion is enhanced by invadopodia and drives invasive behavior. Cell Rep. 5, 1159–1168 (2013).
Bredfeldt, J. S. et al. Computational segmentation of collagen fibers from second-harmonic generation images of breast cancer. J. Biomed. Opt. 19, 16007 (2014).
Stein, A. M., Vader, D. A., Jawerth, L. M., Weitz, D. A. & Sander, L. M. An algorithm for extracting the network geometry of three-dimensional collagen gels. J. Microsc. 232, 463–475 (2008).
Lang, N. R. et al. Estimating the 3D pore size distribution of biopolymer networks from directionally biased data. Biophys. J. 105, 1967–1975 (2013).
This work was supported by the European Research Council (ERC) through the INSILICO-CELL (ERC-2012-StG 306571) project, its proof of concept IMAGO (ERC-PoC-2016-737543) and the Spanish Ministry of Economy and Competitiveness through the project DPI2015-64221-C2-1-R. The authors would also like to thank Microscopy Service of CIBA (IACS- University of Zaragoza). The authors acknowledge Dr. Roger Kamm and his group for their technical assistance during the development of the microfluidic techniques used in this study.
The authors declare no competing interests.
Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Plou, J., Juste-Lanas, Y., Olivares, V. et al. From individual to collective 3D cancer dissemination: roles of collagen concentration and TGF-β. Sci Rep 8, 12723 (2018). https://doi.org/10.1038/s41598-018-30683-4
Clinical & Experimental Metastasis (2021)
Human Cell (2021)
Boiling Histotripsy-induced Partial Mechanical Ablation Modulates Tumour Microenvironment by Promoting Immunogenic Cell Death of Cancers
Scientific Reports (2019)