Translation

Microsystems for Biomechanical Measurements

Abstract

The use of microtechnology to make biomechanical measurements allows for the study of cellular and subcellular scale mechanical forces. Forces generated by cells are in the few nanoNewton to several microNewton range and can change spatially over subcellular size scales. Transducing forces at such small size and force scales is a challenging task. Methods of microfabrication developed in the integrated circuit industry have allowed researchers to build platforms with cellular and subcellular scale parts with which individual cells can interact. These parts act as transducers of stresses and forces generated by the cell during migration or in the maintenance of physical equilibrium. Due to the size and sensitivity of such devices, quantitative studies of single cell and even single molecule biomechanics have become possible. In this review we focus on two classes of cellular force transducers: silicon-based devices and soft-polymer platforms. We concentrate on the biomechanical discoveries made with these devices and less so on the engineering behind their development because this is covered in great detail elsewhere.

Main

Cell-generated forces play an important role in many physiologic processes, and measurements of single cell mechanics are necessary to understand these functions. Microscale systems for force and displacement sensing provide appropriately scaled metrologies for assaying single cells. This review seeks to highlight several opportunities and solutions for single cell measurements and their impact on biology and medicine.

Cells can both generate and sense forces in the extra cellular matrix (ECM) and basement membranes that comprise their three-dimensional in vivo environment. These forces can be transmitted through the ECM proteins or through direct cell-to-cell contact and sensed by neighboring cells. These forces are widely recognized to influence cellular level processes that regulate both normal and pathologic states (13). Forces present in the cellular environment play an important role in events such as wound healing, tissue morphogenesis, and regeneration. Tissue morphogenesis is a complex process involving both spatial and temporal interplays of biochemical factors and mechanical tensions. Tensions present during embryonic development can influence proper growth and organization (48). Tension generation and mechanical force transmission by cells due to migration, stress fiber formation, or active cross-bridging (as in sarcomeres) are of particular interest in diseases having pathologic formation of structural proteins within cells. For example, changes in sarcomeric density, structure, and organization in dilated and hypertrophic cardiomyopathy play a critical role in the contractile properties of cardiac myocytes (CMs) (913). Recent discoveries of large mechanical property changes in red blood cells because of malarial infection have shed light on the molecular pathways involved in the cellular level pathology (14). Fibroblasts migrate into wound areas, and the tension generated by the cells closes the wound and reorganizes the matrix to form scar tissue (15,16). The tension generated in the ECM also acts as a feedback mechanism to regulate fibroblast function (15,17,18). Similarly, studies of the mechanical properties of epithelial cancer cells have raised questions about the role of cell mechanics in cell mobility and metastasis (14). The magnitude and localization of generated forces and how they correlate to cytoskeletal proteins such as actomyosin filaments and the various focal adhesion proteins can provide insight into cellular level pathogenesis. Understanding how the forces are generated, sensed, and transmitted by the subcellular machinery is an important piece of the cell biology puzzle that could help elucidate what goes wrong when tissues fail to form or heal properly.

Studies on tissue mechanics began with the use of traditional materials testing platforms such as tensile stress apparatuses (1921). These devices, however, only provide a macroscale study of the tissue and do not allow isolation of the cellular components from the structural components of a tissue, such as the ECM proteins, nor do they allow for direct measurement of single cells. Single-cell platforms were first developed by scaling two-point tensile-testing methodologies. For example, one of the most common methods for studying myocyte mechanics employs drawn-glass pipettes with a cell glued between the ends. Cell contraction forces are then inferred from the deflection and stress in the pipettes. This method is very time consuming and allows for study of a single cell in each test (2224). Where single-cell, high-throughput platforms for studying cell mechanics are required, devices leveraging Integrated Circuit (IC) industry fabrication methods have been pursued.

Microelectromechanical Systems (MEMS) grew out of IC fabrication for the integration of microscale mechanical features and transducers with electrical components on a single device. Several resources have detailed the fabrication methods and basic MEMS device fundamentals (2529). Using this MEMS toolbox, engineers and biologists have worked together to create several interesting platforms with surface features and force ranges at the scale of single cells (0.1–100 μm and nanoNewtons to microNewtons) (3032). These platforms allow for controlled cell environments where the spatial arrangement of each cell can be defined through the surface topography. This has lead to over two decades of research on how feature size, geometry, and mechanical properties influence cell growth, apoptosis, organization, migration, and differentiation. A great advantage to cell biologists, microsystems can be created at such small scales, and the batch fabrication methods allow for hundreds or thousands of parallel devices on a single platform the size of a standard Petri dish. Such arrays allow data acquisition from each individual cell in an entire population and result in statistically powerful studies.

There are two main classes of microplatforms used for studying the mechanics of cells, silicon-based and polymer-based microsystems. Silicon-based devices created using standard IC methods are designed to contain both moving parts and electrical sensors for observing and recording generated forces. The mechanical parts and the circuitry are matched to the size of a single cell and allow parallel studies of individual cells in a population. These devices are limited in their array size because of the need for electrical interconnects. They also typically require access to a sophisticated fabrication facility with a variety of processes being required such as lithography, plasma etching, and wire bonding. These systems typically lack optical transparency and have limited biocompatibility. However, new materials and surface functionalization can overcome these issues and makes silicon an active area of research for biological studies.

Soft lithography (lithographic fabrication of devices directly in polymers by pattern transfer of silicon) has lead to a new class of force transducers (33). The use of soft polymers such as the epoxy-based resist SU-8, polyacrylamide, poly(dimethyl siloxane) (PDMS), and biological gels such as Matrigel have begun to replace electromechanical devices. Although soft polymer devices are not as amenable to moving parts and integrated electrical circuitry, they are simple to fabricate even in biology labs that may have no MEMS experience. Initial lithographic patterning of silicon wafers to create a master pattern is all that is typically needed. The elasticity of polymers is a better match to cell properties than brittle and stiff silicon. The optical clarity of polymers (vs. opaque silicon) is a property desired by biology researchers who want to correlate cell behavior on the surface with molecular biological processes. Polymer surface chemistry is also readily modified for biocompatibility. In polymer force sensing devices, optically measured displacements of beams (or fluorescent beads in a compliant substrate) are used to infer the forces generated by cells. The small-scale (tens of nanometers) achieved using current fabrication and observation techniques allows for spatial correlation of cell generated forces with cytoskeletal features, focal adhesions, and surface proteins. This subcellular spatial resolution is not readily available with silicon-based force transducers.

In this review, we discuss several microsystem platforms that have been used to study force production and sensing in a variety of cell types. These devices have been divided into categories according to their suitability and application to various biological function related to mechanics, namely traction forces and migration, biochemical pathways, focal adhesion measurements, contraction forces, and stiffness and cytoskeleton. Finally, we discuss a new trend in studying cell mechanics involving embedded sensors and actuators for applying controlled forces to cells. These devices provide new insight to how cells actively respond to the forces they are subject to. This review concentrates on the biological discoveries that have been made, however, given the wide topical area and the limited space, is not comprehensive. For more detail of the analytical and computational methods used, readers are referred to the original articles.

CELL TRACTION AND MIGRATION FORCES

When a cell migrates across a surface, it applies traction forces to that surface. Cell generated traction forces were first investigated by Harris et al. using thin silicone-rubber sheets (34). This method examined wrinkles created on a rubber surface by migrating fibroblasts. Galbraith and Sheetz first used microfabricated silicon cantilever beams to measure traction forces exerted by motile cells like fibroblasts and understand the dynamic force transfer at focal adhesions (Fig. 1) (35,36). The measurements were made with an array of polysilicon cantilevers with pads on the end. The traction forces exerted by the migrating cells as they passed over the pads were inferred from beam deflections which were observed optically. The force resolution was limited by the optical measurement to around 5 nN for a beam stiffness of 75 nN/mm. Observations of fibroblast migration showed forces changed from backward to forward direction between the lamella and the tail of the cell with maximum forces at the tail (+100 nN) an order of magnitude greater than those in the lamellar regions (−5 nN). Immunofluorescence imaging of β1-integrin suggested forces were generated at a small number of focal adhesions. As one of the earliest applications of MEMS in cell biology, this experiment highlighted some of the key features of force generation in migrating fibroblasts. This technique was limited to force measurement in only one direction with spatial resolution equivalent to beam spacing and bandwidth limited by the required postprocessing of video data.

Figure 1
figure1

(A–C). Schematic and images of micromachined array of pads for cell traction force measurement. The migrating cells attach to the pad and the traction forces deflect the embedded lever. The force is inferred from the deflection. D. Schematic of cellular interaction with the pad indicating the direction of the force. Only the forces normal to the direction of the cantilever are measured in this technique. E. A plot of measured forces indicating fluctuations and measurement noise. Images reprinted from Galbraith CG and Sheetz MP, Proc Natl Acad Sci USA 94:9114–9118, Copyright © 1997 National Academy of Sciences, U.S.A., with permission.

The directional and spatial resolution limitations of this technique were overcome by Traction Force Microscopy (TFM) by the incorporation of fluorescent beads into polyacrylamide gel substrates, allowing easy visualization of the deformations created in an elastic substrate through traction forces generated by cells (37) (Fig. 2). Improvements made through the use of time-lapse video-microscopy and improved computational algorithms for determining the deformation field and shear of the substrate opened the way to quantitative measurements of traction forces generated while cells migrate over a surface (38). Surface-attached cells created tension in the polyacrylamide substrate causing deformations that moved the beads from their reference position. This technique involved imaging cells after they have attached and then removing the cells via trypsinization to relax the substrate and get the reference position of the beads. The actual determination of force maps is challenging and requires the use of computationally intensive algorithms for determining the applied forces. TFM has a reported spatial resolution of approximately 4 to 6 μm (3941). Besides polyacrylamide gel, this technique has also been used with gelatin and PDMS substrates (4143). For a more detailed theory behind the computation of traction forces using fluorescent bead substrates, readers are referred to the review by Wang and Lin (44).

Figure 2
figure2

(A). Fluorescent beads embedded in polyacrylamide gel with attached migrating fibroblast (arrow shows direction of migration). (B). Deformation vectors of the substrate. (C). Vector field of traction stresses generated by the cell. (D). Color map showing local magnitude of traction stresses. Image reprinted from Munevar S, et al., Biophys J 80:1744–1757, Copyright © 2001 The Biophysical Society, with permission.

A strength of TFM is the ability to map traction forces over the basal surface of a cell. In mapping traction forces in locomoting fibroblasts, Pelham and Wang observed the greatest forces were found at the front of the migrating cell (39). This finding was contradictory to the behavior in locomotion studies using micromachined silicon cantilevers reported by Galbraith and Sheetz who observed greater traction forces concentrated at the rear of a cell (35). However, different fibroblast types were used in each study and the device by Galbraith and Sheetz had limited directional detection capability, both of which could have contributed to the observed difference.

BIOCHEMICAL PATHWAYS

TFM has been extended to study the effects of various biomolecules and environmental conditions on traction forces: α-smooth muscle actin in myofibrils (45), blebbistatin, a myosin II inhibitor, on migrating fibroblasts (46), α6β4 integrin in carcinoma cells (47,48), phosphorylation of the heat shock protein, HSP27 on the actin cytoskeleton (49), role of electric fields in cellular repositioning (50), and effect of substrate compliance (51). Gaudet et al. showed the influence of collagen concentration on fibroblast migration and found that force generation was dependant on cell area; they estimated the tension in an integrin-collagen bond at 100 pN (52). Using the mapping ability of TFM, Munevar et al. found the front and rear cell-substrate adhesions play different roles during migration; frontal adhesions provide the major force transmission sites whereas rear adhesions play a passive role in anchoring the cell (53). They also observed that 3T3 fibroblasts transfected with the oncogene H-ras had abnormal migratory behavior – including poor directional stability, transient adhesions and increased migratory velocity – behavior associated with metastasis (38).

FOCAL ADHESION FORCES

Two variations of TFM were introduced by Balaban et al. (54). These methods used continuous PDMS sheets, created using soft lithography, to mold the base platform. Instead of randomly distributed fluorescent markers in the bulk of the substrate, the patterns were created on the surface in a precise row-column arrangement. The first method involved creating a regularly arrayed pattern of pits in the surface of PDMS. In the second method, the pattern, also in a regular array, was created using fluorescent photoresist dots embedded in the surface of the PDMS. This had the advantage over traditional TFM in that deformation through application of force was easily monitored, because the markers were placed in a regular array. Any deviation of a marker from this regular array indicated an application of force. The fluorescent marker method has the advantage that the markers are much easier to see under large cells than the pits in the PDMS. Using these platforms, average force for a single fibroblast focal adhesion was found to be 10 nN. There was a positive correlation between force and focal adhesion area; however, the stress at a single focal adhesion was constant at 5.5 nN/μm2. From this, they estimated the force per integrin molecule at 1 pN.

Tan et al. introduced Microfabricated Post Array Detectors (mPADs) as an alternative method to TFM (55). mPADs are PDMS arrays of microposts that have the appearance of a “bed of nails” and act as cantilevers (Fig. 3 A). Cells lie on top of the bed of microposts and once attached, forces generated through stress-fiber formation or contraction will cause deflections of the posts. The posts are created using soft-lithography techniques and provide discrete areas of attachments (i.e., the posts) for the cells. Each of these discrete attachments can be analyzed in isolation from the rest of the substrate, unlike TFM which needs intensive computational algorithms to localize the forces in the continuous substratum to the position of the markers. From beam theory, the deflection of the tip of the micropost has a simple linear relationship to the applied force (Fig. 3 B). The goal is to obtain extremely sensitive microposts (i.e., low-spring constant) such that large displacements are observed from applied forces. The discrete nature of the microposts decouples the generated forces at the point of attachment from the rest of the substrate thereby limiting influence from neighboring cells or posts. Spatial correlation of proteins and microposts can be achieved through immunohistochemical staining. These studies determine which proteins are implicated in force production, how their expression level changes with levels of force production, and how their arrangement influences direction of the forces (Fig. 3 C) (56).

Figure 3
figure3

(A) smooth muscle cell attached to a field of microposts. Tension in the cell bends the posts. (B). Cell stained for visualization of actin (green) and nucleus (blue). Actin bundles are seen to terminate on the tops of the microposts (red). (C). Linear relationship between micropost bending and applied force where D is post diameter, L is length, E is the material's Young's modulus, X is the displacement, and F is the applied force. Images reprinted from Sniadecki NJ and Chen CS, Methods Cell Biol 83:313–328, Copyright © 2007 Elsevier Inc., with permission.

Mechanical characterization of mPADs and how cells interact with the microposts has benefited from the use of finite element analysis. Proper micropost spacing to avoid sagging of cells into the interpost space can be designed (57). Accuracy of the linear model has been tested for various geometries, aspect ratios, and displacement ranges of microposts (57,58). Of course, variations from the ideal columnar geometry due to fabrication tolerances can greatly influence the sensitivity of the micropost. mPADs have been used to study forces generated by motile cells such as fibroblasts, smooth-muscle cells, and epithelial cells (55,5961). Beyond traction force measurements, the discrete nature of the microposts has been invaluable in understanding the role of various proteins in force generation. The role of cadherins, cell-cell junction proteins, has been studied by immobilizing an N-cadherin chimera to the top of microposts (62). Attachment to the microposts through cell-presented cadherins mimics cell-cell contacts. Observed deflection of the posts demonstrated that forces are transmitted through cadherins. Force transmitted through a single cadherin molecule was estimated at 10 pN. The role of cell-cell contacts was also studied in Madin-Darby canine kidney epithelial cells. Interestingly, larger forces were observed in Madin-Darby canine kidney epithelial sheets than in isolated cells suggesting mechanical cooperation between contacting cells (60). When the mechanical properties of the substrate are a determining factor in quantifying cell forces, the stiffness of the sensor may be altering the natural mechanical activity of the cell (63). Focal adhesions on more compliant microposts are less stable and less defined than those on more rigid ones; stiffer microposts also elicit greater forces in epithelial cells (61). Forces were found to be linearly proportional to total adhesion area when focal adhesions were greater than 1 μm2, but forces were much greater when focal adhesions were smaller (55).

CELLULAR CONTRACTION FORCES

mPADs have found application in studying contractile forces of CMs (64,65). Forces were found to be largest parallel to the long-axis of the cell. Application of isoproterenol caused myocytes to increase their force of contraction, resulting in greater displacement of the microposts, thereby demonstrating mPADs use in observation of pharmacologically altered cell function (66). Sarcomeric structure in CMs is intimately related to force production; however, this structure is rapidly lost during in vitro culture (67). Microchannels and large anchoring posts were first shown to maintain neonatal CM morphology and sarcomeric structure by Motlagh et al. (68). Zhao et al. then incorporated these features into mPADs to maintain proper morphology and sarcomeric structure in isolated neonatal CMs (64,68).

A 3D polysilicon based MEMS force sensor for measuring contractile forces in cardiac cells was developed by Lin et al. (Fig. 4) (69,70). The 3D structures were manually assembled with micromanipulators after surface micromachining processes (71). Cardiac cells were glued to the grips attached to cantilever force sensors and contractile forces were inferred from optically observed deflections of the calibrated polysilicon beam structures. The force sensors were miniaturized to a volume less than 1 mm3 and fit into fluidic chambers perfusing biological media. The contractile force of rat heart cells in the presence of CaCl2 activating solution was 12 μN as measured with devices having spring constants around 0.57 N/m. This technique was used in a range of Ca2+ concentrations and the measured forces were fit to a Hill curve. These first MEMS-based measurements of cardiac cells agreed well with pipette-based measurements which often are problematic due to lack of substrate adhesions, cell handling damage, and uncontrolled length variation during contraction (72).

Figure 4
figure4

Schematic of 3D polysilicon force transducer for measuring contraction of heart cell. The cell is held between the rotated plates and the contraction force is measured by the deflection of the calibration flexible beams. Images reprinted from Lin G, et al., IEEE ASME J Microelectromech Syst 9:9–17, Copyright © 2000 Elsevier Inc., with permission.

Cantilevers, as described above, are traditionally made from silicon-based material. Bending of the cantilever may be measured optically by image processing or via a reflected laser spot. Polymer-based cantilevers, however, offer platforms that have a compliance more closely matched to cells, are optically transparent, and are suited for studying actively contracting cells such as cardiomyocytes. Cardiomyocytes attached to the surface of a PDMS cantilever produce bending upon contraction that can be optically measured and quantified (Fig. 5) (73). This method allows for cooperative studies of self-organized CMs on cantilevers with large surface areas able to accommodate multiple cells. Using this system, both in-plane and out-of-plane bending of the cantilever can be monitored. Determination of the forces that result in such deformations have to be determined through extensive image processing and analytical computation or finite element modeling of the cantilever (73,74). To obtain better control of cellular placement and organization on the cantilevers, microgrooves were created on the surface to orient cells lengthwise along the cantilever (Fig. 5 C) (75). These grooves allowed for cells to organize along the long axis of the cantilever so that the majority of generated force went into bending the cantilever along its length. Using flat cantilevers, forces generated by single cardiomyocytes were estimated to be 2 to 5 nN/μm2. This increased to 4 to 7 nN/μm2 on grooved substrates, suggesting an important substrate interaction effect (75).

Figure 5
figure5

(A). Neonatal rat cardiomyocytes cultured on a PDMS cantilever. Reprinted with permission from Anal Chem (73). Copyright 2005, The American Chemical Society. (B). Vertical bending of PDMS cantilever due to applied strain from cells. Reprinted with permission from Conf Proc IEEE Eng Med Biol Soc (74). Copyright 2000, IEEE. (C). Side-by-side flat and grooved PDMS microcantilevers. The grooved cantilever shows greater deflection than the flat cantilever because more stress is applied along the long-axis of the cantilever. Image reprinted from Park J, et al., J Micromech Microeng 16:1614–1619, Copyright © 2006 IOP Publishing Ltd., with permission.

CELL STIFFNESS AND CYTOSKELETON

Saif and coworkers developed a silicon cantilever-based system for studying the mechanics of single cells under large deformation (76,77). This technique was specifically developed to address some of the drawbacks of other methods in measuring stiffness of cells. The force transducers were functionalized with fibronectin to promote adhesion to cells. The external stage was moved to stretch the cell and the deflection of the cantilever tip with respect to the stage was optically observed (Fig. 6). The cell force-deformation curves thus obtained were described by a truss model of cytoskeletal stiffness, with microtubule compression struts and actin tensile fibers (76). The cell deformations were linear and repeatable for large deformations, though linearity and reversibility were lost in the presence of cytochalasin-D, an actin polymerization inhibitor. The responses suggested a reversible polymerization mechanism maintains cell stiffness over many cycles (78). This technique had the specific advantage of measuring large cell deformations, making it useful for understanding cell response to large strain events or injuries. Such measurements can enable an understanding of the physiologic processes involved in defining and maintaining the structure of cells. The calibrated, single-crystal silicon probes used in this work provided some of the most precise, quantitative data reported from cell mechanics studies.

Figure 6
figure6

(A). Schematic of cell stiffness measurement with cantilever deflection and cell deformation. The probe is pulled to a distance R by an external actuator, deforming the cell by D. The force is measured from the calibrated spring stiffness and deflection, w. (B). Force-deflection plot of a cell indicating reversible and repeatable deformation. (B–D). Images of measured cell after probe attachment (B), under small deformation (C) and large deformation (D) corresponding to data in (A). Image reprinted from Yang S and Saif T, Exp Cell Res 305:42–50, Copyright © 2005 Elsevier Inc., with permission.

Sun et al. developed a dual-axis electrostatic actuator system with capacitive displacement sensing for feedback control that was well suited for biomechanical studies of single cells. The system comprised comb-drive electrostatic actuators on a suspended x-y stage, allowing a silicon probe to be manipulated in a plane, and capacitive sensors to measure the displacement (79,80). The system was used to measure the extra-cellular membrane stiffness of zona pellucida oocytes (Fig. 7) (79). The stiff probe entered the cell culture media but the combs remained in air. Mechanical models describing the membrane deformation were fit to measured forces and properties of the cell membrane were extracted.

Figure 7
figure7

(A). Image of dual-axis actuator and capacitive force sensor for cell manipulation studies. The comb-drives are used to actuate the probe and interdigitated capacitances are used for measuring the force in both axes. (B,C). Images of undeformed (B) and deformed (C) mouse oocyte ZP with an applied force of 7.21 μN and deflection of 42.2 μm. Image reprinted from Sun Y, et al., IEEE Trans Nanobioscience 2:279–286, Copyright © 2003 IEEE, with permission.

CONCLUSION

Microsystems technology is promising for various cell mechanics applications. The dimensions, force, and displacement ranges of these devices can be matched to the biological systems under study. For instance, modifications of TFM and mPADs have also been used to study animal locomotion (81). Further, the variety of sensing techniques allows flexible measurement techniques to be tailored for a specific cell type and measurement. Some of the recent progress includes embedding sensors into the force transducers, enabling direct readout of the forces and circumventing elaborate optical setups and image processing (82). This could also lead to higher bandwidth recording for dynamic measurements or integration with patch clamp recordings. Other advances like the development of microactuators in liquid media also have potential applications in controlled application of forces to study cell mechanics (83). New techniques are also being developed that could bridge the gap between IC-based devices and soft-polymer devices. Adding circuitry into soft polymers is an active area of research (84). Incorporation of magnetic particles into mPADs posts has been demonstrated (85). This technique allows for applying forces to the cell, through the micropost, by using magnetic fields.

Advances in fabrication techniques are one way to improve the study of biological phenomena. Another issue that needs to be addressed beyond fabrication is how to study cells, using these techniques, in a manner that is more similar to the in vivo, physiologic state of cells. The described techniques only study cells in a planar or 2D arrangement, but cells grown in 3D gels that more naturally mimic the in vivo environment exhibit changes in growth and function (8689). At present, no techniques have been reported to measure traction forces in individual cells in a 3D environment, but extending these techniques to tri-axial stresses and strains will be important. Studying mechanical activity in 3D in vitro environments will lead to greater insight into how cells behave in their natural state, lead to techniques to be applied in vivo, and may ultimately be able to guide the design of in vitro environments for tissue engineering and regenerative medicine.

Abbreviations

bioMEMS:

biological microelectrical mechanical systems

CM:

cardiomyocyte

ECM:

extracellular matrix

IC:

integrated circuit

MEMS:

microelectrical mechanical systems

mPADs:

microfaricated post array detectors

TFM:

traction force microscopy

PDMS:

poly(dimethyl siloxane)

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Correspondence to James J Norman.

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Norman, J., Mukundan, V., Bernstein, D. et al. Microsystems for Biomechanical Measurements. Pediatr Res 63, 576–583 (2008). https://doi.org/10.1203/PDR.0b013e31816b2ec4

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