Cell traction.

Traction forces are exerted by cells on their substratum as they migrate. These forces under the entire cell or subcellular regions can be measured. This unit describes several protocols for making silicone sheets to measure traction forces under the entire cell, as well as a protocol for developing a micromachined device to measure forces under subcellular regions.

Multiple forces contribute to cell sheet morphogenesis for dorsal closure in Drosophila.

The molecular and cellular bases of cell shape change and movement during morphogenesis and wound healing are of intense interest and are only beginning to be understood. Here, we investigate the forces responsible for morphogenesis during dorsal closure with three approaches. First, we use real-time and time-lapsed laser confocal microscopy to follow actin dynamics and document cell shape changes and tissue movements in living, unperturbed embryos. We label cells with a ubiquitously expressed transgene that encodes GFP fused to an autonomously folding actin binding fragment from fly moesin. Second, we use a biomechanical approach to examine the distribution of stiffness/tension during dorsal closure by following the response of the various tissues to cutting by an ultraviolet laser. We tested our previous model (Young, P.E., A.M. Richman, A.S. Ketchum, and D.P. Kiehart. 1993. Genes Dev. 7:29-41) that the leading edge of the lateral epidermis is a contractile purse-string that provides force for dorsal closure. We show that this structure is under tension and behaves as a supracellular purse-string, however, we provide evidence that it alone cannot account for the forces responsible for dorsal closure. In addition, we show that there is isotropic stiffness/tension in the amnioserosa and anisotropic stiffness/tension in the lateral epidermis. Tension in the amnioserosa may contribute force for dorsal closure, but tension in the lateral epidermis opposes it. Third, we examine the role of various tissues in dorsal closure by repeated ablation of cells in the amnioserosa and the leading edge of the lateral epidermis. Our data provide strong evidence that both tissues appear to contribute to normal dorsal closure in living embryos, but surprisingly, neither is absolutely required for dorsal closure. Finally, we establish that the Drosophila epidermis rapidly and reproducibly heals from both mechanical and ultraviolet laser wounds, even those delivered repeatedly. During healing, actin is rapidly recruited to the margins of the wound and a newly formed, supracellular purse-string contracts during wound healing. This result establishes the Drosophila embryo as an excellent system for the investigation of wound healing. Moreover, our observations demonstrate that wound healing in this insect epidermal system parallel wound healing in vertebrate tissues in situ and vertebrate cells in culture (for review see Kiehart, D.P. 1999. Curr. Biol. 9:R602-R605).

Keratocytes pull with similar forces on their dorsal and ventral surfaces.

As cells move forward, they pull rearward against extracellular matrices (ECMs), exerting traction forces. However, no rearward forces have been seen in the fish keratocyte. To address this discrepancy, we have measured the propulsive forces generated by the keratocyte lamella on both the ventral and the dorsal surfaces. On the ventral surface, a micromachined device revealed that traction forces were small and rearward directed under the lamella, changed direction in front of the nucleus, and became larger under the cell body. On the dorsal surface of the lamella, an optical gradient trap measured rearward forces generated against fibronectin-coated beads. The retrograde force exerted by the cell on the bead increased in the thickened region of the lamella where myosin condensation has been observed (Svitkina, T.M., A.B. Verkhovsky, K.M. McQuade, and G. G. Borisy. 1997. J. Cell Biol. 139:397-415). Similar forces were generated on both the ventral (0.2 nN/microm(2)) and the dorsal (0.4 nN/microm(2)) surfaces of the lamella, suggesting that dorsal matrix contacts are as effectively linked to the force-generating cytoskeleton as ventral contacts. The correlation between the level of traction force and the density of myosin suggests a model for keratocyte movement in which myosin condensation in the perinuclear region generates rearward forces in the lamella and forward forces in the cell rear.

Cell migration as a five-step cycle.

The migration of cells over substrata is a fundamental and critical function that requires the co-ordination of several cellular processes which operate in a cycle. At the level of the light microscope, the cycle can be divided into five steps: (1) extension of the leading edge; (2) adhesion to matrix contacts; (3) contraction of the cytoplasm; (4) release from contact sites; and (5) recycling of membrane receptors from the rear to the front of the cell. Each step is dependent upon one or more cyclical biochemical processes. The development of many in vitro and subcellular assays for the fundamental biochemical processes involved has increased our understanding of each cycle dramatically in the last several years to include a definition of many of the protein and enzymic components, the role of the position of extracellular-matrix receptors on the cell, and the contribution of physical force. The next generation of questions are directed at resolving the roles of the many individual proteins in each step of the cell migration process. In this chapter we will examine each of the migration steps and discuss the biochemical mechanisms that may underlie them.

Forces on adhesive contacts affect cell function.

Cellular forces acting on the adhesive contacts made with the extracellular matrix (ECM) contribute significantly to cell shape, viability, signal transduction and motility. In the past two years, research has determined how cell spreading influences cell viability as well as cytoskeletal organization. The cytoskeleton generates a level of tension against the ECM that is proportional to ECM stiffness. The strength of this tension exerted against the ECM affects the migratory speed of the cell.

Cell migration: regulation of force on extracellular-matrix-integrin complexes.

Cell migration relies upon forces generated by the cell. Recent studies have provided new insights into the processes by which cells generate and regulate the forces applied to extracellular matrix (ECM)-bound integrins and have led us to the working model described here. In this model, ECM binding to integrins in the front of lamellipodia causes those integrins to attach to the rearward-moving cytoskeleton. Integrin-cytoskeleton attachments in the front are strengthened as a result of ECM rigidity, enabling the cell to pull itself forward. The reduction in contact area at the rear compared with that at the lamellipodium concentrates the traction forces in the rear on fewer integrin-ECM bonds, facilitating release. In such a model, cell pathfinding and motility can be influenced by ECM rigidity.

Shear stress induces spatial reorganization of the endothelial cell cytoskeleton.

The morphology of endothelial cells in vivo depends on the local hemodynamic forces. Cells are polygonal and randomly oriented in areas of low shear stress, but they are elongated and aligned in the direction of fluid flow in regions of high shear stress. Endothelial cells in vitro also have a polygonal shape, but the application of shear stress orients and elongates the cells in the direction of fluid flow. The corresponding spatial reorganization of the cytoskeleton in response to the applied hemodynamic forces is unknown. In this study, we determined the spatial reorganization of the cytoskeleton throughout the volume of cultured bovine aortic endothelial cells after the cells had been exposed to a physiological level of shear stress for 0, 1.5, 3, 6, 12, or 24 h. The response of the monolayer to shear stress was not monotonic; it had three distinct phases. The first phase occurred within 3 h. The cells elongated and had more stress fibers, thicker intercellular junctions, and more apical microfilaments. After 6 h of exposure, the monolayer entered the second phase, where the cells exhibited characteristics of motility. The cells lost their dense peripheral bands and had more of their microtubule organizing centers and nuclei located in the upstream region of the cell. The third phase began after 12 h of exposure and was characterized by elongated cells oriented in the direction of fluid flow. The stress fibers in these cells were thicker and longer, and the heights of the intercellular junctions and microfilaments were increased. These results suggest that endothelial cells initially respond to shear stress by enhancing their attachments to the substrate and neighboring cells. The cells then demonstrate characteristics of motility as they realign. The cells eventually thicken their intercellular junctions and increase the amount of apical microfilaments. The time course of rearrangement can be described as a constrained motility that produces a new cytoskeletal organization that alters how the forces produced by fluid flow act on the cell and how the forces are transmitted to the cell interior and substrate.

A micromachined device provides a new bend on fibroblast traction forces.

We have measured the traction forces generated by fibroblasts using a novel micromachined device that is capable of determining the subcellular forces generated by individual adhesive contacts. The front of migrating fibroblasts produced intermittent rearward forces whereas the tail produced larger forward directed forces. None of the forces were steady; they all had periodic fluctuations. The transition between forward and rearward traction forces occurred at the nucleus, not at the rear of the cell or the border between the endoplasm and the ectoplasm. We propose that the coupling of lamella extensions to fluctuating rearward tractions in front of the nuclear region move the front of a fibroblast forward, while force-facilitated release of rear adhesive contacts and anterior-directed tractions allow the region behind the nucleus to advance.