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Mechanobiology in Lung Epithelial Cells: Measurements, Perturbations, and Responses

Christopher M. Waters, Esra Roan, Daniel Navajas

10.1002/cphy.c100090

Source: Volume 2, Issue 1, January 2012

Published online: January 2012

Full Article on Wiley Online Library



Abstract

Epithelial cells of the lung are located at the interface between the environment and the organism and serve many important functions including barrier protection, fluid balance, clearance of particulate, initiation of immune responses, mucus and surfactant production, and repair following injury. Because of the complex structure of the lung and its cyclic deformation during the respiratory cycle, epithelial cells are exposed to continuously varying levels of mechanical stresses. While normal lung function is maintained under these conditions, changes in mechanical stresses can have profound effects on the function of epithelial cells and therefore the function of the organ. In this review, we will describe the types of stresses and strains in the lungs, how these are transmitted, and how these may vary in human disease or animal models. Many approaches have been developed to better understand how cells sense and respond to mechanical stresses, and we will discuss these approaches and how they have been used to study lung epithelial cells in culture. Understanding how cells sense and respond to changes in mechanical stresses will contribute to our understanding of the role of lung epithelial cells during normal function and development and how their function may change in diseases such as acute lung injury, asthma, emphysema, and fibrosis. © 2012 American Physiological Society. Compr Physiol 2:1‐29, 2012.

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Figure 1. Figure 1.

Alveolar distension in lung inflation. An alveolus was imaged at baseline (Palv = 5 cmH2O, green pseudocolor) and hyperinflation (Palv = 20 cmH2O, red pseudocolor). Numbers in baseline image label two perimeter segments. An overlay of the images demonstrates inflation‐induced alveolar expansion, which increased perimeter length and alveolar diameter by 13% and 15%, respectively. Adapted (with permission) from reference 198.
Figure 2. Figure 2.

Diagram of pressures and forces acting on region of lung isolated by a plane transecting lung. A is the area of the transection and ΣFi is the sum of all tensile forces in the tissue elements transecting the plane. Adapted (with permission) from reference 170.
Figure 3. Figure 3.

Model of the disposition of axial, septal, and peripheral fibers in an acinus showing the effect of surface forces (arrows). From reference 285.

Reprinted with permission of the publisher. Copyright © 1984 by the President and Fellows of Harvard College.
Figure 4. Figure 4.

Force balance in the epithelial cell monolayer subjected to in‐plane stretch. Inward tension (red arrows) produced by active contractile tension generated by actomyosin motors and passive elastic recoil exerted by the actin meshwork is counterbalanced by outward adhesive forces (blue arrows) exerted by the adjacent cells and the extracellular matrix.
Figure 5. Figure 5.

Alveolar edema results in the expansion of the air‐filled alveolus and the contraction of the fluid‐filled alveolus. From reference 199.

Reprinted with permission of the American Thoracic Society. Copyright © American Thoracic Society.
Figure 6. Figure 6.

Measurement of cell mechanics with atomic force microscopy. (Top) The atomic force microscope indents the surface of the cell with a flexible cantilever with a sharp tip placed at its end. The cantilever is displaced with a piezoactuator. Force is computed from the lateral displacement on a segmented photodetector of a laser beam reflected on the cantilever. (Bottom) Force‐displacement (F‐z) curve recorded in an alveolar epithelial cell showing the force measured while the cantilever was approached (solid line) toward the cell and retracted (dashed line) at constant velocity (6 μm/s). The curve exhibits hysteresis indicative of viscoelasticity. The retracted limb exhibits unspecific adhesion before the tip‐cell contact was lost (F < 0). The arrow indicates the estimated contact point. Sinusoidal oscillations were applied at a given indentation to compute the complex shear modulus.

Reprinted from reference 4 with permission from Elsevier.
Figure 7. Figure 7.

Magnetic twisting cytometry (MTC). (Top) Scanning electron microscopy of a bead bound to the surface of a human airway smooth muscle (HASM) cell. (Bottom) A magnetic field introduces a torque which causes the bead to rotate and to displace. M denotes the direction of the bead's magnetic moment.

Images reproduced (with permission) from reference 77.
Figure 8. Figure 8.

Optical tweezers. (A) A sketch of optical tweezers‐based cytorheometer. Optical tweezers were used to manipulate an intracellular granular structure (lamellar body, left circle), or an extracellular antibody coated glass bead (right circle). (B) A bright‐field image of lamellar bodies that abundantly exist in alveolar epithelial type II cells.

Reprinted (with permission) from reference 284.
Figure 9. Figure 9.

Mice myoblast stretched with microplates.

Reprinted from reference 60 with permission from Elsevier.
Figure 10. Figure 10.

Microaspiration of adhered cells. The micropipette is gently pressed against the glass slide and slid into contact with the adherent cell (A). A vacuum is applied; aspiration of the cell arrow into the pipette bore (B and C).

Reprinted from reference 32 with permission from Elsevier.
Figure 11. Figure 11.

Spontaneous displacement fluctuations of a microbead attached to the surface of human airway smooth muscle cells. Scale bar = 5 μm.

Reprinted (with permission) from reference 30.
Figure 12. Figure 12.

Measurements of cell tractions exerted to the substrate. (Top) Traction microscopy. Cell tractions exerted by a human airway smooth cell on a polyacrylamide gel coated with collagen. Colors show the magnitude and direction of the traction vectors in pascal. Adapted (with permission) from reference 31. (Bottom) Micropost array. Confocal image of immunofluorescence staining of a smooth muscle cell on posts. Position of fibronectin (red) on the tips of the posts was used to calculate force exerted by cells (white arrows).

Reprinted (with permission) from reference 242. Copyright (2003) National Academy of Sciences, USA.
Figure 13. Figure 13.

Uniaxial stretching device. A strip of silicone is held between the two clamps within the dish.

Reprinted from reference 178 with kind permission from Springer Science+Business Media.
Figure 14. Figure 14.

Cell stretcher based on the inflation of a clamped elastic diaphragm. Human epidermal keratinocytes (NHEKs) plated on a thin polydimethylsiloxane (PDMS) membrane are subjected to biaxial strain when subject to transdiaphragm pressure.

Reprinted from reference 225, Copyright (2007), with permission, from IOS Press.
Figure 15. Figure 15.

In‐plane biaxial cell membrane stretcher coupled to MTC. A flexible‐bottomed well is positioned on a sample holder based on a hollow cylindrical loading post, concentric with the objective of the microscope. The application of a negative pressure underneath the annular outer region of the sample results in a homogeneous and equibiaxial strain of the central area. Two pairs of coaxial coils are coupled to the stretching device to perform MTC. The pair transverse to the sample plane was used to magnetize the beads with a short and strong magnetic pulse. The pair coaxial to the optical axis applied oscillatory twisting fields. Adapted (with permission) from reference 257.
Figure 16. Figure 16.

Device to produce homogenous strains in a cruciform silicone membrane. Adapted (with permission) from reference 279.
Figure 17. Figure 17.

Biologically inspired design of a human breathing lung‐on‐a‐chip microdevice. Application of vacuum to the side chambers causes mechanical stretching of membrane forming the alveolar‐capillary barrier.

Adapted (with permission) from reference 127. Reprinted (with permission) from AAAS.
Figure 18. Figure 18.

Map of selected in vitro experiments utilizing alveolar epithelial cells, immortalized or primary. To distinguish the type of cells utilized in these studies, that is, AEII, A549, and AEI‐like, color coding is utilized as shown in the map. The AEI‐like cells are primary AEII cells that are cultured to four or more days. The reference numbers are given in the boxes and are listed in Table 1.
Figure 19. Figure 19.

Illustration indicating four ways in which the plasma membrane can respond to stretch. Adapted (with permission) from reference 267.
Figure 20. Figure 20.

Progression of an air bubble within the collapsed small airways results in large normal and shear stresses that deform the cells significantly and result in plasma membrane injury. Adapted (with permission) from reference 24.
Figure 21. Figure 21.

Frequency dependence of G′ (A) and G″ (B) under baseline conditions (filled symbols) and during application of a single stretch of 14.1% (open symbols). Data are plotted as means ± SEM. Adapted (with permission) from reference 257.
Figure 22. Figure 22.

Elastic modulus of cells is dependent on the distance from the wound edge in 16HBE cells. (A) Representative elastic modulus map of migrating 16HBE cells at a wound edge 2 h after wounding. Arrows indicate the wound edge as cells were migrating from right to left. Grey regions indicate plastic substrate. (B) Median elastic modulus values as a function of distance from the wound edge were summarized from four different fields. The dashed line indicates the median value from control cells far away from the wound edge (2.4 kPa), and the asterisks indicate a significant difference from this value (P < 0.05). Adapted (with permission) from reference 272.


Figure 1.

Alveolar distension in lung inflation. An alveolus was imaged at baseline (Palv = 5 cmH2O, green pseudocolor) and hyperinflation (Palv = 20 cmH2O, red pseudocolor). Numbers in baseline image label two perimeter segments. An overlay of the images demonstrates inflation‐induced alveolar expansion, which increased perimeter length and alveolar diameter by 13% and 15%, respectively. Adapted (with permission) from reference 198.



Figure 2.

Diagram of pressures and forces acting on region of lung isolated by a plane transecting lung. A is the area of the transection and ΣFi is the sum of all tensile forces in the tissue elements transecting the plane. Adapted (with permission) from reference 170.



Figure 3.

Model of the disposition of axial, septal, and peripheral fibers in an acinus showing the effect of surface forces (arrows). From reference 285.

Reprinted with permission of the publisher. Copyright © 1984 by the President and Fellows of Harvard College.


Figure 4.

Force balance in the epithelial cell monolayer subjected to in‐plane stretch. Inward tension (red arrows) produced by active contractile tension generated by actomyosin motors and passive elastic recoil exerted by the actin meshwork is counterbalanced by outward adhesive forces (blue arrows) exerted by the adjacent cells and the extracellular matrix.



Figure 5.

Alveolar edema results in the expansion of the air‐filled alveolus and the contraction of the fluid‐filled alveolus. From reference 199.

Reprinted with permission of the American Thoracic Society. Copyright © American Thoracic Society.


Figure 6.

Measurement of cell mechanics with atomic force microscopy. (Top) The atomic force microscope indents the surface of the cell with a flexible cantilever with a sharp tip placed at its end. The cantilever is displaced with a piezoactuator. Force is computed from the lateral displacement on a segmented photodetector of a laser beam reflected on the cantilever. (Bottom) Force‐displacement (F‐z) curve recorded in an alveolar epithelial cell showing the force measured while the cantilever was approached (solid line) toward the cell and retracted (dashed line) at constant velocity (6 μm/s). The curve exhibits hysteresis indicative of viscoelasticity. The retracted limb exhibits unspecific adhesion before the tip‐cell contact was lost (F < 0). The arrow indicates the estimated contact point. Sinusoidal oscillations were applied at a given indentation to compute the complex shear modulus.

Reprinted from reference 4 with permission from Elsevier.


Figure 7.

Magnetic twisting cytometry (MTC). (Top) Scanning electron microscopy of a bead bound to the surface of a human airway smooth muscle (HASM) cell. (Bottom) A magnetic field introduces a torque which causes the bead to rotate and to displace. M denotes the direction of the bead's magnetic moment.

Images reproduced (with permission) from reference 77.


Figure 8.

Optical tweezers. (A) A sketch of optical tweezers‐based cytorheometer. Optical tweezers were used to manipulate an intracellular granular structure (lamellar body, left circle), or an extracellular antibody coated glass bead (right circle). (B) A bright‐field image of lamellar bodies that abundantly exist in alveolar epithelial type II cells.

Reprinted (with permission) from reference 284.


Figure 9.

Mice myoblast stretched with microplates.

Reprinted from reference 60 with permission from Elsevier.


Figure 10.

Microaspiration of adhered cells. The micropipette is gently pressed against the glass slide and slid into contact with the adherent cell (A). A vacuum is applied; aspiration of the cell arrow into the pipette bore (B and C).

Reprinted from reference 32 with permission from Elsevier.


Figure 11.

Spontaneous displacement fluctuations of a microbead attached to the surface of human airway smooth muscle cells. Scale bar = 5 μm.

Reprinted (with permission) from reference 30.


Figure 12.

Measurements of cell tractions exerted to the substrate. (Top) Traction microscopy. Cell tractions exerted by a human airway smooth cell on a polyacrylamide gel coated with collagen. Colors show the magnitude and direction of the traction vectors in pascal. Adapted (with permission) from reference 31. (Bottom) Micropost array. Confocal image of immunofluorescence staining of a smooth muscle cell on posts. Position of fibronectin (red) on the tips of the posts was used to calculate force exerted by cells (white arrows).

Reprinted (with permission) from reference 242. Copyright (2003) National Academy of Sciences, USA.


Figure 13.

Uniaxial stretching device. A strip of silicone is held between the two clamps within the dish.

Reprinted from reference 178 with kind permission from Springer Science+Business Media.


Figure 14.

Cell stretcher based on the inflation of a clamped elastic diaphragm. Human epidermal keratinocytes (NHEKs) plated on a thin polydimethylsiloxane (PDMS) membrane are subjected to biaxial strain when subject to transdiaphragm pressure.

Reprinted from reference 225, Copyright (2007), with permission, from IOS Press.


Figure 15.

In‐plane biaxial cell membrane stretcher coupled to MTC. A flexible‐bottomed well is positioned on a sample holder based on a hollow cylindrical loading post, concentric with the objective of the microscope. The application of a negative pressure underneath the annular outer region of the sample results in a homogeneous and equibiaxial strain of the central area. Two pairs of coaxial coils are coupled to the stretching device to perform MTC. The pair transverse to the sample plane was used to magnetize the beads with a short and strong magnetic pulse. The pair coaxial to the optical axis applied oscillatory twisting fields. Adapted (with permission) from reference 257.



Figure 16.

Device to produce homogenous strains in a cruciform silicone membrane. Adapted (with permission) from reference 279.



Figure 17.

Biologically inspired design of a human breathing lung‐on‐a‐chip microdevice. Application of vacuum to the side chambers causes mechanical stretching of membrane forming the alveolar‐capillary barrier.

Adapted (with permission) from reference 127. Reprinted (with permission) from AAAS.


Figure 18.

Map of selected in vitro experiments utilizing alveolar epithelial cells, immortalized or primary. To distinguish the type of cells utilized in these studies, that is, AEII, A549, and AEI‐like, color coding is utilized as shown in the map. The AEI‐like cells are primary AEII cells that are cultured to four or more days. The reference numbers are given in the boxes and are listed in Table 1.



Figure 19.

Illustration indicating four ways in which the plasma membrane can respond to stretch. Adapted (with permission) from reference 267.



Figure 20.

Progression of an air bubble within the collapsed small airways results in large normal and shear stresses that deform the cells significantly and result in plasma membrane injury. Adapted (with permission) from reference 24.



Figure 21.

Frequency dependence of G′ (A) and G″ (B) under baseline conditions (filled symbols) and during application of a single stretch of 14.1% (open symbols). Data are plotted as means ± SEM. Adapted (with permission) from reference 257.



Figure 22.

Elastic modulus of cells is dependent on the distance from the wound edge in 16HBE cells. (A) Representative elastic modulus map of migrating 16HBE cells at a wound edge 2 h after wounding. Arrows indicate the wound edge as cells were migrating from right to left. Grey regions indicate plastic substrate. (B) Median elastic modulus values as a function of distance from the wound edge were summarized from four different fields. The dashed line indicates the median value from control cells far away from the wound edge (2.4 kPa), and the asterisks indicate a significant difference from this value (P < 0.05). Adapted (with permission) from reference 272.

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Article Title: Mechanobiology in Lung Epithelial Cells: Measurements, Perturbations, and Responses
 

How to Cite

Christopher M. Waters, Esra Roan, Daniel Navajas. Mechanobiology in Lung Epithelial Cells: Measurements, Perturbations, and Responses. Compr Physiol 2012, 2: 1-29. doi: 10.1002/cphy.c100090