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Collective cell migration in cohesive units is vital for tissue morphogenesis, wound repair, and immune response. While the fundamental driving forces for collective cell motion stem from contractile and protrusive activities of individual cells, it remains unknown how their balance is optimized to maintain tissue cohesiveness and the fluidity for motion. Here we present a cell-based computational model for collective cell migration during wound healing that incorporates mechanochemical coupling of cell motion and adhesion kinetics with stochastic transformation of active motility forces. We show that a balance of protrusive motility and actomyosin contractility is optimized for accelerating the rate of wound repair, which is robust to variations in cell and substrate mechanical properties. This balance underlies rapid collective cell motion during wound healing, resulting from a tradeoff between tension mediated collective cell guidance and active stress relaxation in the tissue.
Many developmental processes involve collective cell motion, driven by migratory behaviours of individual cells and their interactions with the extracellular environment. An outstanding question is how cells regulate their internal driving forces to maintain tissue cohesiveness while promoting the requisite fluidity for collective motion. Progress has been limited by the lack of an integrative framework that couples cellular physical behavior with stochastic biochemical dynamics underlying cell motion and adhesion. Here we develop a cell-based computational model for collective cell migration during epithelial wound repair that integrates tissue mechanics with active cell motility, cell-substrate adhesions, and actomyosin dynamics. Using this model we show that an optimum balance of protrusive cell crawling and actomyosin contractility drives rapid directed motion of cohesive cell groups, robust to variations in cell and substrate physical properties. We further show that disparate modes of individual cell migration can cooperate to accelerate collective cell migration by fluidizing confluent tissues.
Citation: Staddon MF, Bi D, Tabatabai AP, Ajeti V, Murrell MP, Banerjee S (2018) Cooperation of dual modes of cell motility promotes epithelial stress relaxation to accelerate wound healing. PLoS Comput Biol 14(10): e1006502. https://doi.org/10.1371/journal.pcbi.1006502
Editor: Anand R. Asthagiri, Northeastern University, UNITED STATES
Received: April 26, 2018; Accepted: September 11, 2018; Published: October 1, 2018
Copyright: © 2018 Staddon et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: Data from this study are available at: https://github.com/BanerjeeLab/AAVM/tree/wound_healing.
Funding: SB and MFS acknowledge support from the Institute for the Physics of Living Systems at University College London (UCL), and the Engineering and Physical Sciences Research Council (EPSRC) funded PhD studentship for MFS. SB acknowledges support from UCL Global Engagement Fund. MPM and APT acknowledge funding from Army Research Office Multidisciplinary University Research Initiative W911NF-14-1-0403. MPM also acknowledges funding from the National Science Foundation Civil, Mechanical and Manufacturing Innovation-1525316, and the National Institute of Health U54 CA209992. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Collective cell migration is central to tissue morphogenesis, wound repair and cancer metastasis . During tissue repair after wounding , or during closure of epithelial gaps [3, 4], collective cell migration enables the regeneration of a functional tissue. Gap closure is usually mediated by two distinct mechanisms for collective cell movement [5–7]. First, cells both proximal and distal to the gap can crawl by Arp2/3 driven forward lamellipodial protrusions [6–8]. Secondly, cells around the gap can collectively assemble a supracellular actomyosin cable, known as a purse-string, which closes tissue voids via active contractile forces [6, 9]. It remains poorly understood how these two modes of collective cell movement, driven by the assembly of distinct actin network architectures, are regulated in diverse biophysical conditions.
Many experimental studies have provided key insights into the physical forces driving collective cell migration [7–13]. Recent in vitro wound healing experiments have shown that closure of large wounds is initiated by cell crawling, followed by the assembly of purse string that dominates closure at smaller wound sizes [12, 13]. Purse-string acts like a cable under contractile tension, pulling in the wound edge at a speed proportional to its local curvature . By contrast, crawling driven closure occurs at a constant speed, regardless of wound morphology . However, it remains unknown how the mechanochemical properties of individual cells and their interactions with the extracellular matrix regulate crawling and purse-string based collective cell motion. While experiments are limited in the extent to which mechanical effects are separated from biochemical processes, theoretical and computational models can decouple these variables precisely.
Extensive theoretical work has been done to model collective cell migration during tissue morphogenesis and repair [15–21]. However, existing models do not explain how individual cells adapt their migratory machineries and interactions with neighboring cells to move collectively like a viscous fluid while maintaining tissue cohesion. Continuum models of tissues  as viscoelastic fluids [13, 16] or solids [14, 15, 17, 23] have been successful in describing collective flow and traction force patterns observed experimentally. However, such macroscopic models cannot capture cellular scale dynamics, and therefore unsuited for connecting individual cell properties to collective cell dynamics. On the other hand, cell-based computational models, including the Cellular Potts Model [24, 25], Vertex Model [26, 27], phase-field  or particle-based models [20, 29, 30] explicitly account for dynamic mechanical properties of individual cells and their physical interactions. However, these models have not yet been developed to integrate the mechanics of cell motion with cell-substrate adhesions and intracellular cytoskeletal dynamics. It remains poorly understood how migrating cells sense changes in their physical environment and translate those cues into biomechanical activities in order to facilitate collective motion. This is particularly important for epithelial wound healing, where wound edge cells actively remodel their cytoskeletal machineries and the resulting modes of motility in response to changes in wound size, shapes and substrate properties [12, 14, 31].
To overcome these limitations, we propose an integrative modeling framework that incorporates the mechano-chemical coupling of cell motion and adhesion with stochastic transformation between protrusive and contractile cell behaviors. In contrast to previous cell-based models of wound healing [18, 31, 32], our approach explicitly accounts for the spatiotemporal regulation of protrusive and contractile activities, cell-matrix interactions, adhesion turnover, and cell polarity. Using this model, we ask: How do migrating cells sense changes in their physical environment? How do cells regulate their modes of motilities to optimize the speed of collective motion? What roles do tissue mechanical properties play in stress propagation and relaxation during wound repair? In particular, we find that an optimum mixture of protrusive and contractile cell activities at the wound edge accelerates the rate of wound healing under diverse conditions. The optimum mixed mode of migration is robust to changes in substrate rigidity, wound shape, intercellular adhesions and cortical tension. A unique insight offered by our study is that a mixture of protrusive and contractile activities promotes faster wound repair by optimizing the tradeoff between collective cell guidance and local stress relaxation. Finally, we propose a fundamental mechanism by which tissues can locally fluidize to drive rapid collective cell motion while maintaining their overall mechanical integrity.
Cell-based mechanochemical model
Our model consists of several computational components that simulate: (1) mechanical interactions between cells, (2) biochemical dynamics (protrusions, adhesions), and (3) transitions between distinct cell motility modes. Mechanical interactions between cells are simulated using the vertex model for epithelial mechanics [18, 21, 26, 27, 33–35], where the geometry of each cell is defined by a two-dimensional polygon, with mechanical energy given by: (1)
The first term in (1) represents the energy cost for cell compressibility, where Ai is the area of cell i, A0 is the preferred cell area, and K is the elastic constant. The second term, , is the energy due to contractile forces in the actomyosin cortex. The last term in (1) represents the interfacial tension between cells, which is the difference between cortical tension and the cell-cell adhesion energy per unit length. The elastic substrate is modeled as a triangular mesh of harmonic springs (Methods). Focal adhesion complexes are modeled as stiff springs that anchor the cell vertices to the substrate mesh, with attachment and detachment rates given by kon and koff, respectively (see Methods). The net mechanical force acting on the cell vertex α is given by Fα = −∂Etot/∂xα, where is the total mechanical energy of the cells and the cell-substrate adhesions.
In addition to mechanical forces (Fig 1A), cells within the bulk tissue actively move with a self-propulsion velocity (Fig 1B), where defines the random polarity vector for cell motion, and v0 is the self-propulsion speed. Cells at the wound leading edge initiate motion by crawling towards the wound center [12, 13], with a force fp (Fig 1A). At each time step, crawling cell fronts can transition to a purse-string at a constant rate kp. This leads to an increased line tension on the wound edge due to actomyosin contractility (Fig 1A) (see Methods). Assuming over-damped dynamics, cell vertex α at the wound edge moves as: (2) where μ is the friction coefficient. Cell vertices in the bulk of the tissue move according to following equation of motion (3) where the last term is the averaged self-propulsion force over nα neighboring cells sharing the vertex α (Fig 1B). We estimate the model parameters from available experimental data (Methods, Table 1).
A: Model schematic, showing physical forces and model elements. B: Illustration of self-propulsion force. The central vertex for a cell inside the tissue has a resultant force (red arrow) equal to the average force from its adjacent cells (blue arrows). The polarity vector (blue arrow) for a wound edge cell bisects the angle between the lines from the cell centroid to the boundary vertices. C: Tissue configuration during wound closure with kp = 4 hr−1, at t = 15 min (left), t = 33 min (middle), t = 64 min (right). Arrows indicate traction forces. D-F: Kymograph of the (D) radial component of cell velocity field, vr, (E) magnitude of the azimuthal velocity, |vθ|, and (F) radial traction stress, Tr, for the mixed modality of closure corresponding to (C). G: Log-linear plot for wound area vs time for crawling (kp = 0), purse-string (kp = 1000 hr−1), and mixed (kp = 4 hr−1) modes of closure. Inset: Time evolution of the percentage of wound perimeter covered by purse-string. See Table 1 for the full list of default model parameters.
Cooperation of distinct modes of cell migration during wound repair
To elucidate the mechanisms of collective cell motion during wound repair, we simulated healing of a circular wound for a mixed modality of closure: kp = 4 hr−1. Initially, cells close the wound by crawling (Fig 1C), but over time they switch to the purse-string mode, resulting in rapid contraction of cell edges lining the wound periphery (Fig 1C, S1 Video). To quantify the spatiotemporal patterns of collective cell motion, we calculated spatially averaged radial and azimuthal velocities as a function of the radial distance from the wound center at each time point (Fig 1D and 1E). Initially, both radial and azimuthal velocities are highest around the wound edge and decay with distance inside the monolayer. As crawling cells pull on the substrate, the resultant traction forces point radially outwards and away from the wound (Fig 1C and 1F). Halfway through the closure process, the purse-string fully assembles (Fig 1G-inset) and the traction forces switch to pointing radially inwards (Fig 1F), in quantitative agreement with experimental data . Consistent with experiments, tangential traction stresses are comparable in magnitude with the radial components of the traction stress (S2B Fig). Our model reproduces the experimental observation that focal adhesions are oriented towards the wound center for crawling cells [31, 36] (S3A and S3C Fig). By contrast, purse-string adhesions have a higher probability of orienting tangentially at the leading edge than crawling cells (S3B, S3D and S3E Fig). As closure proceeds, the band of high radial velocities around the wound narrows (Fig 1D), while the azimuthal velocity narrows and decreases around the wound (Fig 1E). This results in more coordinated inward motion of the cells.
Increasing kp from 0 (crawling only) to 1000 hr−1, monotonically increases the proportion of wound perimeter covered by the purse-string over time (Fig 1G-inset). For non-zero values of kp, wound area shrinks in a biphasic manner: an initial slow exponential decay, followed by fast exponential decay, consistent with experimental data . In contrast to the mixed mode of closure (Fig 1C and 1G), the traction forces for crawling mediated closure are always directed radially outwards (S2C Fig), because crawling cells pull on the substrate. While further inside the monolayer the traction forces point radially inwards as the rear end of crawling cells retract via cortical contraction. In purse-string mediated closure, the wound shape remains circular throughout (S2 Video), in contrast to the ruffling morphology observed for crawling cell fronts (S2 Video). Traction forces point into the gap, and increases in magnitude as the wound size gets smaller (S2D Fig). For a fixed set of parameters, we find that a balance of purse-string and crawling mediated closure results in faster wound healing (Fig 1G). To determine how the relative proportion of purse-string and lamellipodia is optimized for rapid collective motion, we turned to examine how the purse-string assembly rate (kp) regulates wound closure time for varying physical properties of the cells, the underlying substrate, wound size and shape.
Mixture of crawling and purse-string based motilities accelerates wound closure independent of substrate rigidity
Since the speed of cell crawling and the magnitude of traction forces are sensitive to substrate rigidity [37, 38], we first investigated the role of substrate stiffness on wound closure time. To this end, we varied the substrate Young’s modulus, Es, and the purse-string assembly rate, kp, for fixed physical properties of the tissue and the wound. We find that wound closure time increases with Es for higher values of kp, but remained insensitive for crawling mediated closure (Fig 2A). Strikingly, there exists an optimum value of kp (corresponding to mixed modality) for any value of Es, which results in minimum closure time (Fig 2A). For fixed kp, strain energy transmitted to substrate decreases monotonically with increasing stiffness for Es > 0.5kPa (Fig 2B) (see Methods for calculation details). For all values of Es and kp, faster wound closure coincides with higher strain energy transmitted to the substrate, signifying a positive correlation between energy cost and the speed of wound healing.
A-B: Dependence of closure time (A) and mean strain energy (B) for different values of substrate stiffness (Es) and kp. Starred cells indicate the fastest wound closure for a given Es with varying kp (PS: kp = 1000 hr−1; C: kp = 0). Each data point corresponds to the average of 5 simulations. C: Pearson’s correlation coefficient, r, between closure time and substrate stiffness, for crawling (kp = 0), purse-string (kp = 1000 hr−1), and mixed (kp = 4 hr−1) modes of closure. The asterisk represents coefficients significantly different from zero (p< 0.05); ** means p< 0.01, and *** means p< 0.001. For each mode, n = 25. D-E: Schematic of purse-string driven (D) and crawling mediated (E) cell motility on an elastic substrate. Blue arrows represent reaction force from the substrate, green (red) arrows represent purse-string (protrusion) driving forces, and black arrows represent cortical contractile forces. F: Effective friction from the substrate on the leading edge of the wound for crawling (kp = 0), purse-string (kp = 1000 hr−1), and mixed (kp = 4 hr−1) modes of migration. Error bars represent standard deviation (n = 5).
Our results agree with experimental findings that wound closure time is not sensitive to changes in substrate stiffness for moderate to high rigidities [31, 36]. On very soft substrates (< 500 Pa), our model predictions are inconsistent with experiments by Anon et al , who showed that crawling-based migration fails to close wounds on very soft gels (∼ 100 kPa), as lamellipodia do not form. This may be captured by implementing additional biochemical feedback mechanisms between protrusive activity and substrate stiffness, beyond the scope of our mechanical model.
As Es is increased, purse-string driven motion slows down. To quantify the dependence of closure time on stiffness, we calculated the Pearson’s correlation coefficient between wound closure time and substrate stiffness for different modes of wound closure (Fig 2C). We find that purse-string based motility slows down with increasing stiffness, with a positive correlation coefficient significantly different from zero (p-value < 0.05). In contrast, crawling based motility and have the least significant correlation coefficient (p-value > 0.05).
The sensitivity of purse-string driven motility to substrate rigidity (Fig 2A and 2C) can be explained by a mechanical force balance argument (Fig 2D and 2E). Purse-string driven contractile forces drag the border cells into the gap, in competition with cortical tension retracting the rear cell edges. This results in a large net resistive force from the deforming elastic substrate (Fig 2D). By contrast, crawling cells pull the substrate backwards at the wound edge and contractile forces pull the substrate forward at the cell rear (Fig 2E). This dipole-like traction pattern results in a net assistive force from the substrate, pointing towards direction of cell crawling. During mixed mode of migration, a combination of net assistive and resistive forces should therefore lead to the least sensitivity to substrate stiffness.
To test this hypothesis, we computed the net radial traction force, Fr, on the substrate under the first row of cells at the wound edge. We then calculate the time-averaged ratio between the radial force and the radial velocity, vr, of the wound edge, to obtain an effective friction coefficient: μeff = 〈Fr/vr〉 (Fig 2F). We find that μeff monotonically increases in magnitude with increasing substrate stiffness (for all modes of migration), consistent with previous theoretical predictions . For all values of substrate stiffness, purse-string motion leads to the highest positive μeff, suggesting high resistance and sensitivity to substrate rigidity. Crawling driven motility leads to negative μeff, indicative of assistive motion. By contrast, the mixed mode of migration leads to the lowest magnitude of μeff, i.e. least drag from the substrate.
Rigidity sensing by different modes of collective migration is expected to be strongly coupled to focal adhesion kinetics. While we have assumed constant rates of binding and unbinding of cell-substrate adhesions, experiments have demonstrated that integrin-ligand pairs form catch bonds , such that koff decreases under low forces and increases under larger forces. To test if the mechanosensitivity of cell-substrate adhesion bonds impact our results, we implemented a catch bond model for adhesions, assuming a single bound state and two unbinding pathways  (see Methods). As a result, the crawling mode of closure is now more sensitive to changes in substrate stiffness, with closure time increasing with stiffness, before decreasing at higher stiffnesses due to increased adhesion lifetime (S4 Fig). Purse-string driven closure shows an increase in sensitivity compared to the default case, while the mixed mode of closure is least sensitive to changes in substrate stiffness. However, the mixed mode of migration is always the fastest, irrespective of force sensitivity of the adhesions.
Aside from mechanosensitivity of different modes of wound closure, the driving force for closure is expected to be strongly dependent on the relative proportion of purse-string and crawling cells. Since actomyosin purse-string is a cable under tension, the driving force for closure is proportional to the wound curvature. As a result, purse-string driven closure is expected to be sensitive to the wound geometry [12, 14]. By contrast, crawling driven closure has been found to reduce wound area at a constant speed . Therefore, we sought to investigate how the coaction of purse-string and crawling based motilities modulate collective motion for varying wound morphologies.
Wound geometry regulates the optimum modality of collective motion
For circular wounds of varying radii we recapitulate the experimental result that closure time increases with wound radius (Fig 3A) . However, the optimum purse-string assembly rate (kp) for fastest closure decreases with wound radius, such that closure time is highly sensitive to kp for larger wounds. This is because purse-string driven forces are higher near the end of closure, and that purse-string force is low in the beginning of closure of a large wound. For larger wound radii, an optimum mixture of purse-string and protrusive cell crawling leads to fastest closure. We find that the average strain energy on the substrate increases monotonically with wound radius for kp (Fig 3B), but is more sensitive to wound size for purely crawling mediated migration (kp = 0).
A: Closure time for different values of wound radius and kp. B: Mean strain energy vs wound radius for different values of kp. C: Closure time for different values of wound aspect ratio and kp. D: Substrate strain energy as a function of wound aspect ratio and kp. E: Wound closure time for concave wound shapes for crawling (kp = 0), purse-string (kp = 1000 hr−1), mixed (kp = 4 hr−1) and curvature-sensing modes of closure. Error bars represent standard error of mean (n = 5). F: Velocity against curvature during simulations of the right most shape in (E) for crawling, purse-string and mixed modes of closure. G: Evolution of wound morphology during closure by (i) pure crawling, (ii) pure purse-string, (iii) a combination of crawling and purse-string, and (iv) curvature-dependent formation of purse-string. Colors progressively change from black to red with increasing time.
Next we simulated elliptical shaped wounds of fixed area but varying aspect ratios. We find that regardless of the migratory mode, closure time decreases with increasing aspect ratio (Fig 3C). In addition, there exists an optimum value of kp for a given aspect ratio that leads to minimal closure time. Thus, a mixed mode of closure is always the fastest, but isn’t much faster than crawling mediated closure for high aspect ratio wounds. This is because crawling cells advance at a constant speed perpendicular to the wound edge. Therefore only the short axis distance must be crossed for the wound to close (S4 Video) (S5A Fig). For purse-string driven closure, the high curvature ends of elliptical wounds move rapidly inwards, leading to faster closure than circular shapes (S5C Fig). At all values of aspect ratio, strain energy is inversely proportional to closure time (Fig 3D).
Since purse-string behaves as a contractile cable, then for wounds with concave morphologies (positive curvatures), cells should be pulled away from the wound by the purse-string tension. To investigate this we simulated concave wound shapes as in ref. . For varying degrees of concavity (with fixed area), we observed that a mixed mode of closure leads to fastest wound closure (Fig 3E). To quantify the relationship between wound healing speed and curvature, we measured the local velocity and curvature at the wound perimeter. We find that the purse-string velocity is proportional to the curvature, crawling velocity is curvature-independent, while a mixture of crawling and purse-string leads to faster collective motion, with velocity decreasing with curvature (Fig 3F, S5 Video). These findings quantitatively agree with experimental data .
Previous studies suggest the possibility that purse-string and lamellipodia-based migration during wound healing can be geometrically coupled [14, 29, 31], such that the formation of protrusive borders may be directly coupled to the assembly of purse-string cables on neighboring wound edges with opposite curvatures. Such a mechanism is not captured by a purely stochastic transition between protrusive and contractile activities. To this end, we implemented a model of curvature sensing motility of the wound leading edge, similar to Ref. , where the switching between crawling and purse-string mechanisms is regulated by the local curvature of the wound (S7 Fig). Based on this model, if the curvature of a cell’s leading edge is larger than a threshold curvature, it contracts via purse-string. Otherwise, the cell moves via protrusive crawling (Methods, S7 Fig). We applied this model to wounds with non-uniform curvatures as in Fig 3E. Consequently, the convex regions move forward by crawling, whereas contractile purse-string cables assemble in the concave regions. We find that for all three concave shapes in Fig 3E, the curvature sensing mechanism closes the wound at least as fast as in the mixed case with stochastic switching of motility modes (Fig 3E–3G). We note that the curvature-sensing mechanism may not be applicable to the closure of undamaged epithelial gaps where purse-string cables do not form .
Optimum balance of protrusive and contractile cell activities promotes rapid wound healing via active stress relaxation
Our cell-based model predicts many differences in collective cell motility driven by contractile and protrusive activities (Figs 1–3). In particular, purse-string tension rounds the wound edge and leads to solid-like, radial deformation of the tissue (Fig 3F-inset). By contrast, crawling cells ruffle the wound leading edge (Fig 3G, S3 and S5 Videos), suggestive of lack of guided motion. To quantify differences in tissue deformation and their relationship to collective motion, we measured the angle (θ) between cell center velocity and the unit vector pointing towards the wound center (Fig 4A). In purse-string driven closure (kp = 1000 hr−1), the angle distribution shows a single peak at θ = 0, corresponding to radially inward deformation (Fig 4B). By contrast, crawling cells (kp = 0) have a wider distribution of angles, with secondary peaks at θ = ±π (Fig 4B), representing outward motion from cell neighbor exchanges (Fig 4A). To quantify the distributions, we define collective cell guidance, , as the probability that a cell moves towards the wound center: , which monotonically increases with increasing kp (Fig 4C).
A: Definition of the angle θ between the cell center velocity and the radial vector to wound center. Right: Representative cell velocity fields for crawling and purse-string modes of closure. B: Probability density distribution for θ for crawling (kp = 0), purse-string (kp = 1000 hr−1), and mixed (kp = 4 hr−1) modes of closure. C: Guidance parameter for different values of shape parameter p0 and kp. D: Rate of T1 transitions in the wounded tissue for varying p0 and kp. E: Closure time for different values of p0 and kp. Starred cells indicate the fastest wound closure for a given p0.
Since tissue deformation properties depend on cortical tension, cell contractility, and cell-cell adhesions [34, 42–44], we investigate how cellular mechanical properties regulate collective guidance (). We can rewrite the mechanical energy of cells (Eq (1)) as: (4) where P0 = −γ/2Γ is the preferred cell perimeter. The non-dimensional shape parameter controls cell shape anisotropy and the emergent rigidity of confluent tissues . Increasing p0 reduces cortical tension relative to cell-cell adhesions, which softens the tissue. It has been shown that confluent tissues behave like a jammed solid for p0 < 3.81, whereas it exhibits fluid-like behaviour for p0 > 3.81 . Activity in the form of cell motility, division, or death can fluidize tissues further by lowering the critical p0 for rigidity transition [46–48]. In our model, activity arises from self propulsion (v0) (S1B and S8 Figs), and cell crawling whose relative strength is regulated by kp. We find that increasing p0 decreases , regardless of kp (Fig 4C). The decrease in with increasing p0 arises from an increased rate of cellular neighbor exchanges (T1 transitions) that locally fluidizes the tissue (Fig 4D). Surprisingly, for a fixed p0, T1 rates in the wounded tissue is highest for intermediate values of kp, resulting in minimum closure time (Fig 4E). With higher p0, cells have a higher preferred perimeter, such that both contractile and protrusive motilities experience lower mechanical resistance from tension in the border cells (S6 Video) (S9 Fig). This enables a faster reduction in wound area as compared to rigid tissues with lower p0 (Fig 4E).
These findings elucidate the mechanical basis for rapid collective migration via a mixture of protrusive and contractile cell activities. Purse-string driven tension maximizes collective cell guidance and leads to the lowest frequency of tissue rearrangements, such that cell movements are impeded by mechanical resistance from the surrounding tissue. By contrast, purely crawling motion exhibits the lowest collective guidance due to randomized protrusions of individual cells at the wound leading edge. We find that an optimum mixture of crawling and purse-string leads to intermediate collective guidance, while maximizing the frequency of local tissue rearrangements (Fig 4D). This mechanism of active fluidization enables tissues to locally relax their mechanical stress, promoting rapid wound healing. When intercalations are disabled in the model, tissue mechanical energy increases due to increase in cell elongation around the wound (S10 Fig). This results in cell jamming and slowing down of wound closure. Therefore, cell intercalations, promoted by a mixture of contractile and protrusive forces, lead to efficient wound closure by minimizing both tissue mechanical energy and wound closure time. Recent experiments, however, suggest that cells may not necessarily try to minimize energy or closure time during wound healing . But rather, they tend to coordinate the assembly of diverse actin architectures to conserve the amount of mechanical work done per unit time.
Our cell-based computational model quantitatively captures a wide range of experimental trends including the patterns of collective cell motion and traction stress organization for crawling and purse-string mediated wound closure (Fig 1). We reproduced the experimentally observed size-dependence of wound closure times, the curvature dependence of purse-string velocity, and independence of cell crawl speeds to variations in wound morphology. We predict that increasing aspect ratio of the wound speeds up closure as crawling cells can rapidly cross the short axis of the wound, whereas purse-string cables can generate rapid movements on regions of high curvature (Fig 3).
Robust to variations in substrate and tissue mechanical properties, we find that an optimum proportion of protrusive and contractile motilities accelerates wound closure. While purse-string driven motion slows down on stiffer gels due to an increased resistance from drag on the substrate, crawling driven migration is largely independent of substrate stiffness (Fig 2). We find that a mixed mode of collective migration is more efficient regardless of substrate stiffness. Robust to parameter variations, an increase in closure speed is associated with an increase in the strain energy transmitted to the underlying substrate (S11 Fig). As a result, migrating cells actively dissipate more mechanical energy to their environment in order to speed up collective motion.
A source of active stress dissipation comes from cellular neighbor exchanges that locally fluidize the tissue, resulting in faster wound closure (Fig 4). These T1 transitions have previously been observed in vivo, during wound closure in Drosophila embryo epidermis . T1 transitions are also observed in our in vitro laser-ablation experiments on MDCK monolayers, where the number of cells at the wound edge decreases over time via wound edge intercalations (S12 Fig). In our model, the mechanism of active fluidization via intercalation is promoted by a mixture of protrusive and contractile activities of wound edge cells, and reduced contractility or increased cell-cell adhesion in the bulk of the tissue. The ability to actively remodel an elastic tissue, coupled with tension-driven collective cell guidance, constitute the two key mechanisms for rapid directed motion in adherent environments. While the stress relaxation mechanism in our model comes only from cell neighbor exchanges, other dissipative mechanisms can also be triggered by mechanical forces including cell shape fluctuations , cell division  or cell death . In these cases, our prediction will remain very similar, with the rate of cell movement into free space augmented by the sum of relaxation rates of various dissipation modes . A future challenge is to identify the molecular pathways that activate distinct stress relaxation modes during tissue development and regeneration.
We model the substrate as a triangular mesh of springs with a spring constant ks. The Young’s modulus of the substrate is given by , where hs is the substrate thickness, and the Poisson’s ratio for a triangular mesh is ν = 1/3.
Since focal adhesions and cellular traction forces typically localize at the cell periphery , we implement adhesions at the cell boundaries. We model the focal adhesion complexes as stiff springs with stiffness kf, which connect the cell vertices with the substrate mesh. Bound focal adhesions can detach stochastically with a rate koff, whereas unbound cell vertices can attach to the nearest node of the substrate mesh with a rate kon. The resultant force on the cell vertex is, (5) (6) where , is the adhesion energy, σα is the state variable for cell-substrate attachment (0: detached; 1: attached), rα is the position of the substrate mesh connected to xα, and and are the initial positions of the cell and the substrate vertices at the time of adhesion formation.
Active cell motility
Each cell carries a unit polarity vector, , which represents the front/rear polarization of a motile cell . The polarity vector is an internal state variable of cell that specifies the preferred orientation of cell motion, not their actual direction of motion. Cells in the bulk of the tissue, i.e. not on the wound edge, move due to self-propulsion . The polarity of a bulk cell i is defined by a unit vector with angle θi that undergoes rotational diffusion: (7) where Dr is the rotational diffusion constant, and ηi(t) is a Gaussian white noise with mean 0 and variance 2Dr. The self-propulsion of cell i results in a force on the vertex α as: , where v0 is the self-propulsion speed, and the sum is over all neighboring cells to vertex α (S1B Fig).
Here, we have neglected alignment interactions between cell polarity vectors in the bulk of the tissue, which can drive coherent swirling motion of cell collectives . Without such polarity alignment rules, cell velocity vectors remain correlated over ∼ 5 cell diameters due to mechanical interactions (S13 Fig), somewhat less than the correlation lengths measured in experiments in the absence of a wound .
To model lamellipodia based crawling, we allow cell vertices at the wound edge to protrude in the direction of polarity before attaching to the substrate (S1 Fig). This pushes the cell front outwards, while cortical tension pulls the rear of the cell forwards. The polarity vector of cells along the wound points into the gap, and is determined by the mid-point of the wound edges. The direction of protrusion is given by the unit vector of wound cell i, which makes half the angle between the two lines joining the centroid of cell i to the vertices on the wound that neighbour other cells, i.e. are on the boundary of internal and external edges (S1C Fig). This ensures contact inhibition of locomotion , preventing collision of two neighbouring cells. For a cell i neighbouring the wound, the crawling force on vertex α on the wound edge is given by: , where fp is the protrusion force magnitude. For simplicity we have assumed that fp is independent cell-substrate adhesions. However, protrusive activity remains strongly correlated to focal adhesion kinetics, since the frequency of the protrusions is slaved by the rate of focal adhesion binding and unbinding. As a consequence of this feedback, increasing the duty ratio of adhesions leads to slower crawl speeds and increased closure time (S4D Fig).
Curvature sensing model for purse-string formation
Here we describe the model where the switching between crawling and purse-string modes is dependent on the local geometry of the wound leading edge. At each time step in the simulation, cells at the wound edge makes a decision to switch its motility phenotype based on the local curvature of the wound edge. We calculate the curvature of a wound edge cell as the inverse of the radius of a circle inscribed to that cell edge. Curvature is defined as positive if the wound is convex (e.g. a circle), and negative otherwise. If the curvature is above a threshold value, then the cell switches to a purse-string mode. If the curvature is below the threshold value, then the cell moves by crawling. As a result, cells typically start by crawling and switch to the purse-string mode as the wound shrinks in size, consistent with experimental findings .
To determine the optimum value of the threshold curvature, we varied the threshold curvature for switching to a purse-string mode, and computed the resultant wound closure time for a given initial wound shape. The optimum threshold curvature is given by the curvature value that minimizes wound closure time, as shown in S7B Fig.
Catch bond model for cell-substrate adhesions
The functional form for the detachment rate is taken from a catch bond model for integrin-ligand bonds that assumes a single bound state and two unbinding pathways . The parameters k0, k1, f0, and f1 have previously been estimated for single integrin ligand bonds . Based on that estimate, we calibrate these parameters for the coarse-grained adhesion bonds in our simulations that represent several ligand-integrin pairs. We used parameter values of k0 = 25 hr−1, k1 = 0.006 hr−1, f0 = 3.125 μN, and f1 = 0.6944 μN, which results in the default unbinding rate at zero force, and showed high sensitivity to substrate stiffness.
The vertex model is implemented using Surface Evolver . We generate a wound by removing any cells that lie totally or partially within the wounded area. Edges surrounding the wound are then moved to the target wound shape. We then relax the energy of the remaining cells without adhesions so that all vertices on the wound lie on the target wound perimeter and system is at an energy minimum. To initiate gap closure, cells around the wound are set to crawling mode. We then execute the following steps (S1 Fig) until wound closure:
- Update adhesion states for cell vertices. Adherent vertices attempt to unbind with a rate koff at each time step. Detached vertices attempt to attach to the nearest node of the substrate mesh with a rate kon. For cell edges at the wound border, attachment occurs via protrusion into the nearest substrate vertex.
- Refine cell edges by subdividing edges longer than a maximum length, and merging edges shorter than a minimum length. This ensures an even distribution of adhesions, and allows the cells to assume curved shapes.
- Perform neighbour exchanges, also known as T1 transitions, when a cell edge shrinks below the threshold length, L*, such that it lowers the total mechanical energy. Once an edge goes below the threshold length L*, then that edge is replaced by a perpendicular contact of the same length.
- Update modes of cell movement. Cells at the wound edge switch from crawling to purse string modes at a rate kp. In the purse-string mode, cells can no longer crawl but instead carry a higher line tension around their wounded edge, γps, modelling contractility of the actomyosin cable. Once cells are in the purse-string mode they remain so until wound closure or when the cell edge length shrinks to zero.
- Move the cell vertices according to the overdamped equation of motion (Eqs (2) or (3)). Individual nodes of the substrate spring mesh move at a velocity proportional to the net force resulting from focal adhesions and the gradient of mechanical energy of the spring mesh.
Table 1 lists the parameters used in our simulations. The number of cells was chosen to be large enough to avoid finite size effects and displacement on the outer row of the cells. To confirm this, we ran wound healing simulations using different numbers of cells. As the number of cells increases from 50, closure time increases and then quickly plateaus after cell count reaches 100 (S14A Fig). We use a default value of 150 cells, but increase the cell number (in the range 150-250) while running simulations for wounds with larger sizes (Fig 3A). Substrate node density was chosen to be small enough so that a cell vertex is always close to a node in the substrate spring mesh, allowing focal adhesions to form with a relatively short length. As shown in S14B Fig, we find little dependence of closure time on node density, and use 0.6 μm−2 as the default value.
The preferred area of the cell, A0, is chosen to be approximately the same as the average area of MDCK cells in wound healing assays [13, 31]. The preferred perimeter P0 is chosen so that the cell shape index, is close to the value for a regular hexagon, enabling us to study the effects of cell shape anisotropy on wound healing speed. The substrate stiffness was chosen as a typical value for gels used in in vivo wound healing assays ; the Poisson’s ratio of 1/3 for the substrate is a consequence of using a triangular mesh of linear springs. The Young’s modulus of the substrate defines the force scale in the simulations. The wound radius was chosen to be in the range 5-30 μm, similar to those in experimental studies [12, 13, 31].
Purse-string tension was estimated by taking the product of the force generated by a single myosin motor, 3 pN , with the typical number of myosin motors in a contractile ring of length 15 μm and thickness 1 μm, 105 , which gives a tension of 300 nN. Next, we fit parameters for cell area and perimeter elasticities, K and Γ, adhesion binding and unbinding rates, koff and kon. Together, these parameters determine the overall tissue motility and the magnitude of traction force generation. Thus we fit them simulataneously to the experimental data for typical closure speed and traction force magnitudes generated during closure [12, 13, 31]. In addition, we examine the spatiotemporal pattern of traction forces generated during closure. For example, traction stresses are normally localized around the wound but are not evenly distributed around the perimeter. Low adhesion time leads to smooth closure but little traction force while higher adhesion binding times lead to an even distribution of traction around the wound but the closure dynamics are less smooth.
We estimate the protrusion force, fp, by comparing to single cell crawling speeds of 15 μm hr−1 . To this end, we simulated a single crawling cell with a fixed polarity vector, and calibrated fp to the value that resulted in a crawl speed of 15 μm hr−1. Internal motility speed was set to a similar value as cell crawling speeds. Dependence of wound closure time for variations in fp and γps are shown in S2F Fig. Whereas, the dependence of closure time on internal motility, v0 is shown in S8A and S8C Fig. The range of purse-string assembly rates were chosen so that the minimum value, kp = 0 yields pure crawling, the maximum, kp = 1000 hr−1, yields 100% purse-string coverage, and intermediate values produce a combination of purse-string and crawling.
Traction stress computation
We record displacements of the substrate mesh, u = r − r0, at each timestep during the simulation. These vectors are then interpolated to a square grid, from which strain is evaluated using the finite difference discretization of: , where k and l are in-plane spatial coordinates. The resultant stress is: (9)
The traction stress is calculated using Tk = hs∂l σkl. The computed traction force vectors in the square grid are in excellent agreement with forces directly inferred from spring displacements in the triangular mesh (S15 Fig). The strain energy density is given by . For each simulation we calculate the mean strain energy as total strain energy transmitted to the substrate averaged over simulation time, T: (10)
In vitro wound healing experiments
Madin-Darby Canine Kidney (MDCK.2) cells (CRL-2936; ATCC, Manassas, VA) were cultured in Eagle’s Minimum Essential Medium (ATCC) containing 10% fetal bovine serum (GIBCO Life Technologies) and 1% penicillin/streptomycin at 37°C and 5% CO2 in a humidified incubator. MDCK.2 cells are stably transfected with a plasmid construct encoding for FTRActinEGFP (a gift from Sergey Plotnikov, University of Toronto).
Polyacrylamide gels are polymerized onto a glass coverslip at a ratio of 12%:0.086% polyacrylamide:bis-acrylamide to create a gel with an elastic modulus of 12.2 kPa . After polymerization is complete, the polyacrylamide gels are reacted with 2mg/mL Sulfo-SANPAH (Thermo Fisher Scientific) and incubated with 1mg/mL Type 1 rat tail collagen (Corning, high concentration) for 2 hours in the dark . Excess collagen is removed by rinsing with 1X Phosphate-buffered saline.
Confluent cell monolayers were grown on a polyacrylamide gel substrate with an elastic modulus of 12.2 kPa. Wounds were formed by laser ablation of a single cell using a 435 nm wavelength laser (Andor Technology, Belfast, Northern Ireland). Cell death causes monolayer retraction for ∼20 min after which the wounds close.
S1 Fig. Computational pipeline in the wound healing assay.
A: From left to right: 1) Update adhesion states for cell vertices. Adherent vertices attempt to unbind with a rate koff, and unbound vertices attempt to bind to the nearest substrate mesh with a rate kon. 2) Update cell modes from crawling (red) to purse-string (green) with a probability kpΔt. 3) Protrude cell edges in crawling mode (red arrows) and contract cell edges on purse-string mode (green arrows). 4) Minimize mechanical energy to move the cell vertices down their mechanical energy gradient (black arrows). B: Illustration of self-propulsion force on a vertex in the bulk. The central vertex has a resultant force (red arrow) equal to the average force from its adjacent cells (blue arrows). C: The polarity vector (blue arrow) for a cell around the wounds bisects the angle between the lines from the cell centroid to the boundary vertices (dashed lines).
S2 Fig. Forces driving wound closure.
A: Traction stress distribution around a closing wound with kp = 4 hr−1, at t = 5 min (left), t = 30 min (middle), t = 60 min (right). B: Kymograph of tangential traction stress for the mixed mode of closure (kp = 4 hr−1). C: Kymographs of radial and tangential traction stress for the crawling (kp = 0 hr−1) mode of closure. D: Kymographs of radial and tangential traction stress for the purse-string (kp = 1000 hr−1) mode of closure. E: Total strain energy transmitted vs time for crawling, purse-string, and mixed modes of closure. F: Closure time as a function of purse-string tension (green) and protrusion force (red) for a mixed mode of closure (kp = 4 hr−1). Error bars represent standard error of mean.
S3 Fig. Orientation of cell-substrate adhesions in leading edge cells.
Histograms of the local angle between cell-substrate bonds and the radial vector to the wound center, in (A) crawling and (B) purse-string cells at the leading edge. (C) Representative image of crawling cells with focal adhesions oriented normal to the wound edge. (D) A purse-string edge flanked between two crawling edges have its focal adhesions parallel to the wound edge. (E) Purse-string only wounds have a majority of adhesions oriented normal to the wound edge, due to normal driving forces arising from contractile tension in the purse-string. Green segments represent purse-string edges, while red segments are crawling cells.
S4 Fig. Effect of cell-substrate adhesion kinetics on wound closure time.
(A) Mean adhesion lifetime, , vs applied force for a catch-bond model (blue) and constant koff (yellow). (B) Substrate stiffness dependence of wound closure time for a catch-bond model of cell-substrate adhesions, for crawling (red), purse-string (green) and mixed (kp = 4 hr−1, black) modes of closure. (C) Wound closure time vs substrate stiffness for constant koff. Each data point represent average over 6 simulations. Error bars show standard deviation. (D) Closure time vs duty ratio of focal adhesion bonds, kon/(koff + kon), for crawling, purse-string and mixed modes of wound closure. Duty ratio is varied by changing the detachment rate, koff, for a fixed kon.
S5 Fig. Shape dependent dynamics of wound closure.
Wound morphologies for (A) crawling (kp = 0 hr−1), (B) mixed (kp = 4 hr−1), and (C) purse-string (kp = 1000 hr−1) modes of closure, at t = 6 min (left), t = 18 min (middle), t = 30 min (right). The initial aspect ratio of the wound is 4.
S6 Fig. Dependence of traction stress on cell, substrate and wound properties.
Temporal mean of spatially averaged traction stress during wound closure for different values of kp and (A) substrate stiffness, (B) wound radius, (C) wound aspect ratio, and (D) shape parameter p0.
S7 Fig. Model for curvature dependent purse-string formation.
(A) Schematic showing purse-string and crawling edges for a wound with non-uniform curvature. Purse-string (PS; green) forms on leading edges with curvature κ > κ*, where κ* is a threshold curvature. Cells prefer to crawl (C; red) if κ < κ*. (B) Wound closure time vs κ* for the concave shaped wound in (A). The optimum threshold curvature is chosen to be the one that minimizes wound closure time. Dashed lines indicate wound closure times for pure crawling (red), pure purse-string (red) and stochastic mixed (black) modes of closure.
S8 Fig. Internal motility accelerates the rate of wound closure.
(A) Closure time, and (B) mean strain energy for different values of internal motility v0 and kp. Starred cells indicate the fastest wound closure for a given v0 with varying purse-string assembly rates. (C) Closure time, and (D) average strain energy for different values of shape parameter p0 and internal motility v0, for a mixed mode of closure (kp = 4 hr−1).
S9 Fig. Tissue morphology prior to wound closure for different values of shape parameter p0, from 3.0 (solid-like tisue) to 4.0 (fluid-like tissue).
S10 Fig. Intercalations reduce tissue mechanical energy.
(A) Total tissue mechanical energy vs time, with intercalations enabled and disabled during wound closure. (B) Mean cell shape parameter vs time. Shaded regions represent one standard deviation. With intercalations disabled, cells elongate and have more variability in shape. (C-D) Simulation image showing tissue morphology before closure with intercalations (C), and in a jammed state without intercalations (D). Cells are much more elongated when intercalations are disabled. (E) Total substrate strain energy, and (F) total focal adhesion strain energy, over time with intercalations enabled and disabled.
S11 Fig. Faster closure leads to higher strain energy transmitted to the substrate.
Mean strain energy vs closure time. Each data point represents a different simulation. The color corresponds to the parameter that was being varied in that simulation.
S12 Fig. Intercalation events can occur during wound healing.
(A) Time-lapse images of fluorescent F-actin within MDCK cells closing a wound and (B) the drawn outlines of cells initially at the leading edge. Cells at the leading edge at each time point are numbered in red, whereas cells excluded from the leading edge during closure are numbered in cyan. (C) The probability distribution of fractional cell loss for N = 18 wounds where the average number of cells initially at the leading edge is 9 ± 2. N = 8 wounds exhibit a loss of cells at the leading edge during closure. Within this subset, the average percentage of cells lost is 0.23 ± 0.14. (C-inset) The closure timescale, τ, calculated from A(t) = A(0)e−t/τ, where A(t) is the area of the wound at time t, vs the fractional cell loss at the leading edge.
S13 Fig. Velocity-velocity correlation of cells during wound closure.
Figure shows velocity-velocity correlation function, Cvv(r) = 〈v(0).v(r)〉/〈v(0)2〉, where r is the distance between two cell center velocity vectors, v. Cvv(r) is shown at different time points (indicated by color) for (A) crawling, (B) purse-string, and (C) mixed modes of wound closure. Velocity vectors of cells on opposite sides of the wound are anti-correlated.
S14 Fig. Dependence of wound closure time on cell count and substrate node density.
Closure time vs (A) cell count, (B) density of nodes in the substrate spring mesh, for a wound of fixed initial size.
S15 Fig. Comparison of traction force computation methods.
Figure shows traction force vectors using two different methods computed during wound closure at t = 30 min (left column), t = 36 min (middle column), and t = 42 min (right column). (A) Traction force vectors computed using the continuum elasticity Eq (9). (B) Continuum model based forces in (A) interpolated on the substrate triangular mesh. (C) Traction forces directly computed from displacements in the substrate spring mesh. (D) Error map showing the difference of traction force vectors in (B) and (C). Lengths of arrows are proportional to the magnitude of the traction force, and the scale is consistent between images.
S1 Video. Wound healing driven by a mixture of crawling and purse-string.
S2 Video. Wound healing driven by pure purse-string.
S3 Video. Wound healing driven by pure cell crawling.
S4 Video. Wound closure simulations for a circular and an elliptical wound.
S5 Video. Wound closure simulations for a concave wound shape.
- 1. Friedl P, Gilmour D. Collective cell migration in morphogenesis, regeneration and cancer. Nature reviews Molecular cell biology. 2009;10(7):445. pmid:19546857
- 2. Grose R, Hutter C, Bloch W, Thorey I, Watt FM, Fässler R, et al. A crucial role of β1 integrins for keratinocyte migration in vitro and during cutaneous wound repair. Development. 2002;129(9):2303–2315. pmid:11959837
- 3. Jacinto A, Woolner S, Martin P. Dynamic analysis of dorsal closure in Drosophila: from genetics to cell biology. Developmental Cell. 2002;3(1):9–19. pmid:12110163
- 4. Rosenblatt J, Raff MC, Cramer LP. An epithelial cell destined for apoptosis signals its neighbors to extrude it by an actin-and myosin-dependent mechanism. Current Biology. 2001;11(23):1847–1857. pmid:11728307
- 5. Begnaud S, Chen T, Delacour D, Mège RM, Ladoux B. Mechanics of epithelial tissues during gap closure. Current Opinion in Cell Biology. 2016;42:52–62. pmid:27131272
- 6. Martin P, Lewis J. Actin cables and epidermal movement in embryonic wound healing. Nature. 1992;360(6400):179–183. pmid:1436096
- 7. Anon E, Serra-Picamal X, Hersen P, Gauthier NC, Sheetz MP, Trepat X, et al. Cell crawling mediates collective cell migration to close undamaged epithelial gaps. Proceedings of the National Academy of Sciences. 2012;109(27):10891–10896.
- 8. Fenteany G, Janmey PA, Stossel TP. Signaling pathways and cell mechanics involved in wound closure by epithelial cell sheets. Current Biology. 2000;10(14):831–838. pmid:10899000
- 9. Bement WM, Forscher P, Mooseker MS. A novel cytoskeletal structure involved in purse string wound closure and cell polarity maintenance. The Journal of Cell Biology. 1993;121(3):565–578. pmid:8486737
- 10. Trepat X, Wasserman MR, Angelini TE, Millet E, Weitz DA, Butler JP, et al. Physical forces during collective cell migration. Nature physics. 2009;5(6):426.
- 11. Tambe DT, Hardin CC, Angelini TE, Rajendran K, Park CY, Serra-Picamal X, et al. Collective cell guidance by cooperative intercellular forces. Nature materials. 2011;10(6):469. pmid:21602808
- 12. Vedula SRK, Peyret G, Cheddadi I, Chen T, Brugués A, Hirata H, et al. Mechanics of epithelial closure over non-adherent environments. Nature Communications. 2015;6:6111. pmid:25608921
- 13. Cochet-Escartin O, Ranft J, Silberzan P, Marcq P. Border forces and friction control epithelial closure dynamics. Biophysical Journal. 2014;106(1):65–73. pmid:24411238
- 14. Ravasio A, Cheddadi I, Chen T, Pereira T, Ong HT, Bertocchi C, et al. Gap geometry dictates epithelial closure efficiency. Nature Communications. 2015;6.
- 15. Sherratt JA, Martin P, Murray J, Lewis J. Mathematical models of wound healing in embryonic and adult epidermis. Mathematical Medicine and Biology: A Journal of the IMA. 1992;9(3):177–196.
- 16. Lee P, Wolgemuth CW. Crawling cells can close wounds without purse strings or signaling. PLoS Computational Biology. 2011;7(3):e1002007. pmid:21423710
- 17. Banerjee S, Utuje KJ, Marchetti MC. Propagating stress waves during epithelial expansion. Physical Review Letters. 2015;114(22):228101. pmid:26196647
- 18. Nagai T, Honda H. Computer simulation of wound closure in epithelial tissues: Cell–basal-lamina adhesion. Physical Review E. 2009;80(6):061903.
- 19. Salm M, Pismen L. Chemical and mechanical signaling in epithelial spreading. Physical biology. 2012;9(2):026009. pmid:22476663
- 20. Basan M, Elgeti J, Hannezo E, Rappel WJ, Levine H. Alignment of cellular motility forces with tissue flow as a mechanism for efficient wound healing. Proceedings of the National Academy of Sciences. 2013;110(7):2452–2459.
- 21. Mirams GR, Arthurs CJ, Bernabeu MO, Bordas R, Cooper J, Corrias A, et al. Chaste: an open source C++ library for computational physiology and biology. PLoS Computational Biology. 2013;9(3):e1002970. pmid:23516352
- 22. Banerjee S, Marchetti MC. Continuum models of collective cell migration. arXiv preprint arXiv:180506531. 2018;.
- 23. Köpf MH, Pismen LM. A continuum model of epithelial spreading. Soft Matter. 2013;9(14):3727–3734.
- 24. Graner F, Glazier JA. Simulation of biological cell sorting using a two-dimensional extended Potts model. Physical review letters. 1992;69(13):2013. pmid:10046374
- 25. Albert PJ, Schwarz US. Dynamics of cell ensembles on adhesive micropatterns: bridging the gap between single cell spreading and collective cell migration. PLoS Computational Biology. 2016;12(4):e1004863. pmid:27054883
- 26. Honda H, Eguchi G. How much does the cell boundary contract in a monolayered cell sheet? Journal of Theoretical Biology. 1980;84(3):575–588. pmid:7431941
- 27. Farhadifar R, Röper JC, Aigouy B, Eaton S, Jülicher F. The influence of cell mechanics, cell-cell interactions, and proliferation on epithelial packing. Current Biology. 2007;17(24):2095–2104. pmid:18082406
- 28. Löber J, Ziebert F, Aranson IS. Collisions of deformable cells lead to collective migration. Scientific reports. 2015;5:9172. pmid:25779619
- 29. Tarle V, Ravasio A, Hakim V, Gov NS. Modeling the finger instability in an expanding cell monolayer. Integrative Biology. 2015;7(10):1218–1227. pmid:26099063
- 30. Zimmermann J, Camley BA, Rappel WJ, Levine H. Contact inhibition of locomotion determines cell–cell and cell–substrate forces in tissues. Proceedings of the National Academy of Sciences. 2016;113(10):2660–2665.
- 31. Brugues A, Anon E, Conte V, Veldhuis JH, Gupta M, Colombelli J, et al. Forces driving epithelial wound healing. Nature Physics. 2014;10(9):683–690. pmid:27340423
- 32. Nagai T, Honda H. Wound healing mechanism in epithelial tissues cell adhesion to basal lamina. WSEAS Transactions on Biology and Biomedicine. 2006;3(6):389.
- 33. Fletcher AG, Osterfield M, Baker RE, Shvartsman SY. Vertex models of epithelial morphogenesis. Biophysical Journal. 2014;106(11):2291–2304. pmid:24896108
- 34. Manning ML, Foty RA, Steinberg MS, Schoetz EM. Coaction of intercellular adhesion and cortical tension specifies tissue surface tension. Proceedings of the National Academy of Sciences. 2010;107(28):12517–12522.
- 35. Staple D, Farhadifar R, Röper JC, Aigouy B, Eaton S, Jülicher F. Mechanics and remodelling of cell packings in epithelia. The European Physical Journal E. 2010;33(2):117–127.
- 36. Ajeti V, Tabatabai AP, Fleszar AJ, Staddon MF, Seara DS, Suarez C, et al. Epithelial Wound Healing Coordinates Distinct Actin Network Architectures to Conserve Mechanical Work and Balance Power. arXiv preprint arXiv:180606768. 2018;.
- 37. Discher DE, Janmey P, Wang Yl. Tissue cells feel and respond to the stiffness of their substrate. Science. 2005;310(5751):1139–1143. pmid:16293750
- 38. Schwarz US, Safran SA. Physics of adherent cells. Reviews of Modern Physics. 2013;85(3):1327.
- 39. Walcott S, Sun SX. A mechanical model of actin stress fiber formation and substrate elasticity sensing in adherent cells. Proceedings of the National Academy of Sciences. 2010;107(17):7757–7762.
- 40. Kong F, García AJ, Mould AP, Humphries MJ, Zhu C. Demonstration of catch bonds between an integrin and its ligand. The Journal of Cell Biology. 2009;185(7):1275–1284. pmid:19564406
- 41. Pereverzev YV, Prezhdo OV, Forero M, Sokurenko EV, Thomas WE. The two-pathway model for the catch-slip transition in biological adhesion. Biophysical Journal. 2005;89(3):1446–1454. pmid:15951391
- 42. Foty RA, Steinberg MS. The differential adhesion hypothesis: a direct evaluation. Developmental Biology. 2005;278(1):255–263. pmid:15649477
- 43. Mertz AF, Banerjee S, Che Y, German GK, Xu Y, Hyland C, et al. Scaling of traction forces with the size of cohesive cell colonies. Physical Review Letters. 2012;108(19):198101. pmid:23003091
- 44. Mertz AF, Che Y, Banerjee S, Goldstein JM, Rosowski KA, Revilla SF, et al. Cadherin-based intercellular adhesions organize epithelial cell–matrix traction forces. Proceedings of the National Academy of Sciences. 2013;110(3):842–847.
- 45. Bi D, Lopez J, Schwarz J, Manning ML. A density-independent rigidity transition in biological tissues. Nature Physics. 2015;11(12):1074.
- 46. Ranft J, Basan M, Elgeti J, Joanny JF, Prost J, Jülicher F. Fluidization of tissues by cell division and apoptosis. Proceedings of the National Academy of Sciences. 2010;107(49):20863–20868.
- 47. Bi D, Yang X, Marchetti MC, Manning ML. Motility-driven glass and jamming transitions in biological tissues. Physical Review X. 2016;6(2):021011. pmid:28966874
- 48. Barton DL, Henkes S, Weijer CJ, Sknepnek R. Active Vertex Model for cell-resolution description of epithelial tissue mechanics. PLoS Computational Biology. 2017;13(6):e1005569. pmid:28665934
- 49. Razzell W, Wood W, Martin P. Recapitulation of morphogenetic cell shape changes enables wound re-epithelialisation. Development. 2014;141(9):1814–1820. pmid:24718989
- 50. Curran S, Strandkvist C, Bathmann J, de Gennes M, Kabla A, Salbreux G, et al. Myosin II controls junction fluctuations to guide epithelial tissue ordering. Developmental cell. 2017;43(4):480–492. pmid:29107560
- 51. Wyatt TP, Harris AR, Lam M, Cheng Q, Bellis J, Dimitracopoulos A, et al. Emergence of homeostatic epithelial packing and stress dissipation through divisions oriented along the long cell axis. Proceedings of the National Academy of Sciences. 2015;112(18):5726–5731.
- 52. Szabó A, Ünnep R, Méhes E, Twal W, Argraves W, Cao Y, et al. Collective cell motion in endothelial monolayers. Physical Biology. 2010;7(4):046007. pmid:21076204
- 53. Schaumann EN, Staddon MF, Gardel ML, Banerjee S. Force localization modes in dynamic epithelial colonies. bioRxiv. 2018; p. 336164.
- 54. Angelini TE, Hannezo E, Trepat X, Fredberg JJ, Weitz DA. Cell migration driven by cooperative substrate deformation patterns. Physical Review Letters. 2010;104(16):168104. pmid:20482085
- 55. Oakes PW, Bidone TC, Beckham Y, Skeeters AV, Ramirez-San Juan GR, Winter SP, et al. Lamellipodium is a myosin-independent mechanosensor. Proceedings of the National Academy of Sciences. 2018;115(11):2646–2651.
- 56. Brakke KA. The surface evolver. Experimental Mathematics. 1992;1(2):141–165.
- 57. Miyata H, Yoshikawa H, Hakozaki H, Suzuki N, Furuno T, Ikegami A, et al. Mechanical measurements of single actomyosin motor force. Biophysical Journal. 1995;68(4 Suppl):286S. pmid:7787092
- 58. Biron D, Alvarez-Lacalle E, Tlusty T, Moses E. Molecular model of the contractile ring. Physical Review Letters. 2005;95(9):098102. pmid:16197254
- 59. Yeung T, Georges PC, Flanagan LA, Marg B, Ortiz M, Funaki M, et al. Effects of substrate stiffness on cell morphology, cytoskeletal structure, and adhesion. Cell motility and the Cytoskeleton. 2005;60(1):24–34. pmid:15573414
- 60. Sabass B, Gardel ML, Waterman CM, Schwarz US. High resolution traction force microscopy based on experimental and computational advances. Biophysical Journal. 2008;94(1):207–220. pmid:17827246