Introduction

Intricate multi-scale interactions among cells, tissues, and organs fundamentally govern human health, which has evolved on Earth under a constant gravitational load of 1 g (9.8 m/s2). The biological mechanisms underlying the role of gravity in human health remain poorly understood, but their elucidation is necessary for enabling long-term manned space exploration. Numerous studies, supported by the National Aeronautics and Space Administration and other space agencies, have shown deleterious effects of space travel on the human body, such as accelerated bone loss,1,2 muscle tissue degeneration,3 and others.4 Importantly, these observations may have broader implications beyond spaceflight applications to provide a more detailed understanding of diseases on Earth. In particular, the musculoskeletal system has historically been a focal point in space biology research, because of the strikingly adverse changes that occur in astronauts.5 More recently, studies have begun to investigate mesenchymal stem cells for their roles in musculoskeletal lineage determination,6 bone repair,7 and tissue maintenance.8

Although the most relevant environment for performing microgravity research is in space, competition to use space-based facilities, like the International Space Station, is fierce and is further complicated by substantial time and resource investments.9 As a result, lower-cost and logistically simpler alternatives are attractive and include sounding rockets10 and parabolic flights,11 or in-lab devices such as random positioning machines12 and clinorotation devices (clinostats)13 to simulate microgravity. The selection of a specific technique usually depends on accessibility, cost, experimental design, and research question. Clinostats are among the most accessible methods to simulate microgravity, and they allow researchers to study living cells using standard laboratory tissue culture supplies.14

Clinorotation experiments have provided significant insight into the behavior of biological organisms in space. The technique was originally developed to study gravitropism in plant development, and has revealed that gravity serves a key role in statocyte function, which is believed to be directly involved in plant gravisensing and growth patterns.15 In animal and human cells, clinorotation has been used to recreate experiments that would otherwise be challenging to perform in space, such as high-resolution microscopy16 and assessment of stem cell differentiation.17 Cellular changes in microgravity have been associated with disruptions in the cytoskeleton and, consequently, changes in cell morphology and behavior.18,19

Although clinorotation is a standard ground-based tool, previously reported studies on the effects of simulated microgravity in mesenchymal stem cells have yielded conflicting findings (Table 1). For instance, some researchers have shown that microgravity enhances proliferation,17 whereas others have demonstrated inhibition.20 Chondrogenic differentiation has also been found to be either promoted21 or suppressed.22 Similar inconsistencies have also been highlighted in a recent review.23 Some of these observed discrepancies could be due to differences in culture media formulation and cell source, but it is also possible that the choice of clinorotation parameters used for an experiment may substantially influence cell behavior.

Table 1 Previously reported studies on mesenchymal stem cells under simulated microgravity
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A two-dimensional clinostat rotates a sample along the longitudinal axis to produce a time-averaged nullification of the gravity vector. Theoretically speaking, to simulate microgravity effectively, the period of rotation should be shorter than some time constant that governs the rate processes involved in the cellular gravisensing machinery that enable a cell to ‘perceive’ and respond to the changing trajectory of the gravity vector. For conventional clinostats, however, there are also practical considerations that limit the angular frequency of rotation.24 Specifically, rotation speed must be adjusted to balance sedimentation forces, centrifugal and Coriolis effects, and Stokes’ drag. Because of these constraints, the parameters of angular rotation depend on the particular design and implementation of each experimental system.

To minimize the effects of these extrinsic stimuli, we recently developed a lab-on-chip clinorotation device (clinochip, Figure 1a) that confines adhered cells within a small region along the axis of rotation, limiting residual accelerations to levels below 10−4g at different rotation speeds.25 Moreover, the clinochip is amenable to time-lapse microscopy, which enables us to characterize the kinetics of cell spreading, changes in morphology, and migration with minimal disruption to the simulated microgravity environment. In this study, we used this device to investigate how angular frequency affects human mesenchymal stem cell (hMSC) behavior. On the basis of the concept that there are specific rate processes that govern cellular gravisensing (Figure 1b), we hypothesize that hMSCs would exhibit angular frequency-dependent responses. The results of this work demonstrate that hMSCs can in fact ‘detect’ differences in rotation speed in a manner that causes heterogeneous population shifts toward more rounded morphologies and retraction of cell area. This could have significant implications on our basic understanding of stem cell regulation as well as on strategies that are being used in stem cell-based applications.

Figure 1
figure 1

Framework of how perceived gravity may bias cellular events under clinorotation. (a) The clinochip system consists of a stationary non-rotated control chip and a rotating clinochip, the speed of which can be controlled. (b) In the rotating cell-fixed frame of reference, the components of force caused by the gravity vector oscillate in a sinusoidal fashion during clinorotation. Lightly shaded blocks illustrate hypothetical time constants required for various intrinsic cellular events to occur. Forces experienced by cells are shaded in darker colors to help clarify the idea that slower clinorotation (upper graph) may fail to nullify gravity biases for some cell events, whereas faster clinorotation (lower graph) could provide greater probability of nullification for any given event.

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Materials and methods

Materials

hMSCs were obtained from a commercial source (PT-2501, Lonza, Walkersville, MD, USA), and confirmed to be mycoplasma-free. Clinochip fabrication required microscope slides (12-544-1, Fisher Scientific, Waltham, MA, USA) and 0.25- mm-thick polydimethylsiloxane sheets (HT-6240, Rogers Corporation, Rogers, CT, USA). Fluorescence visualization was performed for actin using 5% (w/v) Texas red phalloidin (Life Technologies, Gaithersburg, MD, USA) and for focal adhesions using 1 μg/ml fluorescein-conjugated anti-vinculin (MA1–34629, Life Technologies). Fibronectin (354008, BD Biosciences, San Jose, CA, USA) was used to enable cell adhesion, and nerve growth factor (NGF; 7S-NGF, Life Technologies) was used for migration experiments. Calcein-AM and ethidium homodimer-1 (L-3224, Life Technologies) were used to perform cell viability assays.

Experimental setup

In general, we used a single experimental system for all of our experiments, as detailed previously.25 In brief, the system consists of a custom microscope-mounted gear system, driven by a computer-controlled stepper motor that rotates a small slide holder.25 This slide holder can accommodate various custom and commercially available lab-on-chip devices. A non-rotating slide holder enables having a static (standard gravity) control condition performed concurrently. The entire system is enclosed in an environmental chamber (Precision Plastics, Beltsville, MD, USA) and installed on an Olympus IX-81 epi-fluorescence microscope (Center Valley, PA, USA).

Cell morphology platform

A custom ‘clinochip’ device was used for visualizing cell spreading (that is, changes in cell morphology over time), and fabricated according to our previously described protocol.25 This clinochip consists of three layers comprising polydimethylsiloxane sandwiched between two layers of glass. In brief, we used a high-resolution razor cutter (FC8000, Graphtec, Irvine, CA, USA) to trim stock polydimethylsiloxane sheets. The sheet was cut to length and width dimensions of microscope slides and with a single 1-mm wide, 30-mm long channel at the center. A second microscope slide was used as the third layer. Prior to assembly, two 1-mm diameter holes had been made in the top slide using a sandblaster (6500, Airbrasive, Piscataway, NJ, USA) to provide access to the channels. The three layers were energetically bonded using a high-frequency corona treater (BD-20AC, Electrotechnic Products, Chicago, IL, USA).

The clinochip was first sterilized for 20 min in a UV chamber. To promote cell attachment, the channel was then treated with 100 μg/ml fibronectin for 1 h and washed with phosphate-buffered saline before use. Passage 3 (P3) and P4 hMSCs were seeded into clinochip channels and incubated at 37 °C for 10 min to allow for cell attachment, followed by commencement of clinorotation.

Cell migration platform

Cell migration was analyzed using commercially available Ibidi Chemotaxis slides (μ-Slide Chemotaxis 2D, Ibidi, Munich, Germany). The slides fit perfectly in our clinorotation device and the 2×1 mm dimensions of the chamber are suitable for simulated microgravity, as they constrain cells to a narrow region about the axis of rotation to minimize centrifugal effects. First, a 100 μg/ml fibronectin solution was injected into the viewing chamber and incubated for 1 h, followed by three phosphate-buffered saline washes. Then, P3 and P4 hMSCs were plated and incubated at 37 °C for 12 h of initial seeding time. Our pilot experiments showed that after 12 h the spreading areas of hMSCs reach a plateau so that cell spreading would not confound the cell migration data. As a first step, we chose to study hMSC chemotaxis mediated by NGF, one of several growth factors identified in this active field of research.26 Mesenchymal stem cells have been shown to express receptors to neurotrophic factors including NGF,27 and also secrete NGF during tissue repair.28 In these migration experiments, NGF was prepared as a 100 ng/ml solution and injected into the top ports of the chamber. Following manufacturer’s instructions, the same volume was aspirated from the opposite port to create a chemical gradient.

Clinorotation and time-lapse imaging

Both morphology and chemotaxis platforms were rotated along the axis of the channels in which cells were cultured. Residual accelerations are one to two orders of magnitude smaller than conventional clinostats, even at 75 rpm.25 Before the experiment, we made sure that the channels did not contain any bubbles, to minimize any other external effects such as shear stress and dehydration. During imaging, we constrained our analyses to cells near the axis of rotation, away from the sides of the channel, to avoid potential edge effects.

At the appropriate times (10 min after seeding for morphology assays; 12 h after seeding for chemotaxis and migration assays to allow the cells to become fully spread), clinorotation was initiated at 30, 60, or 75 rpm and maintained over the course of 8 h. Clinochips at 0 rpm (non-rotated) were used as a control (standard gravity). During each hour, rotation was paused for a total of 60 s, and a set of bright-field images of the clinochip were acquired at ×200 magnification. At the end of the 8 h period, cells were fixed in 4% paraformaldehyde, and fluorescently stained for actin and vinculin. Captured images were analyzed using ImageJ (National Institutes of Health).

Cell viability and recovery after clinorotation

Cell viability was determined using calcein-AM (green) to indicate intracellular esterase activity for live cells and ethidium homodimer-1 (red) to indicate loss of plasma membrane integrity for dead cells. Calcein (final concentration 4 μM) and ethidium homodimer (final concentration 2 μM) were added to cell culture media that was used to plate hMSCs in fibronectin-treated clinochips. After 10 min of attachment, clinochips were either rotated at 75 rpm or maintained at standard gravity conditions (non-rotated control) and fluorescence micrographs were taken at 1, 4, and 8 h during clinorotation.

In addition to the live/dead assays, we acquired light micrographs of cell morphology in standard gravity following exposure to (a) 1 or 4 h of 30 rpm clinorotation, (b) 1 or 4 h of 60 rpm clinorotation, or (c) 1, 4, or 8 h of 75 rpm clinorotation. After termination of the clinorotation treatment, images were acquired in standard gravity every 30 min for 4 h, and then analyzed for cell area and shape factor using ImageJ (National Institutes of Health).

Statistical analyses

Because no prior publications have quantified cell areas during clinorotation, we relied on pilot data for descriptive statistics to make sample size calculations. Assuming a critical significance level of α=0.05, statistical power of 0.9 (β=0.1), and a detectable difference equal to the population s.d., we performed a power analysis to calculate an estimated sample size of n=23, using the method of Sokal and Rohlf.29 To ensure adequate statistical power for cell area measurements, we chose to include at least n=30 for each sample group (Table 2), acquired over several experimental replicates. All data are expressed as mean±s.e.m. Variance did not markedly differ between groups (less than fourfold). Average cell areas among different clinorotation speeds were first log transformed to improve normality. Differences between clinorotation groups were then statistically analyzed using the Welch’s t-test for samples with unequal variance and unequal sample size, with Tukey post hoc tests for multiple pairwise comparisons.

Table 2 Number of cells measured for each condition in each experiment
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Using Welch's t-test for samples with unequal variance and sample size, we analyzed differences in cell velocity and directionality between 0 (n=15) and 75 rpm (n=6) only for cells that were actively migrating. Similarly, we used Welch's t-test with Tukey post hoc test for multiple pairwise comparisons to analyze differences in cell area between 30 and 75 rpm (at 0, 1, 2, 3, and 4 h) only for cells that were actively retracting (n=28).

Results

Simulated microgravity affects cell spreading

Simulated microgravity had a profound effect on both the extent and kinetics of cell spreading (Figure 2). After the initial 10-min cell attachment and before rotation commenced, all of the groups possessed similar cell areas of ~500 μm2. We found that hMSCs in the non-rotated 0 rpm condition (i.e., standard gravity) markedly increased spreading areas within 1 h after plating, reaching an average of 2000 μm2. Their spreading area increased gradually with time, until they reached an average of 3000 μm2 by 8 h. For clinorotated groups, cell spreading was impeded almost immediately. At 1 h, cells in the 30 rpm group were significantly smaller than control with an average cell area slightly above 1000 μm2; cells at 60 and 75 rpm were both significantly different from 0 and 30 rpm, remaining rounded and small. The effects of clinorotation continued to affect cell spreading over the course of the entire 8 h experiment in a rotation speed-dependent manner. By 8 h, we measured a statistically similar but smaller average area of 2750 μm2 for cells at 30 rpm. In contrast, the 60 rpm group had an average area of 2192 μm2, and the 75 rpm group had the lowest cell area of 1500 μm2, both statistically smaller than 0 and 30 rpm.

Figure 2
figure 2

Human mesenchymal stem cell (hMSC) spreading areas in simulated microgravity. (a) Time analysis of cell spreading of hMSCs in simulated microgravity at different rotation speeds (0, 30, 60, and 75 rpm). Note that increasing the rotation speed resulted in less-spreading area over time. NS Indicates statistically similar average areas (P>0.05). (b) Representative micrographs of hMSCs spreading in a glass substrate coated with FN at different rotation speeds for 8 h (0, 30, 60, and 75 rpm). Note that cells at a speed of 30 rpm were more similar to control, whereas cells at 60 and 75 rpm have adopted a more rounded morphology.

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From a kinetics perspective, the time required for cell spreading areas to reach 2000 μm2 was within 1 h for non-rotating controls, within 4 h for 30 rpm, and within 8 h for 60 rpm. Our experiments did not run long enough to determine whether or not cells would reach this mark for the 75 rpm condition, but based on the observed trends, it appears that cell spreading no longer increases after 7 h. These results indicate that cell spreading is markedly affected by angular frequency and that these effects can be observed as soon as 1 h after clinorotation starts. Finer temporal resolutions and longer durations in future experiments may provide more detailed insight on the time constant of important cellular processes associated with cellular gravisensing.

One notable observation we made was that cells within each clinorotation speed were not uniformly spread. As individual cells did not accurately represent the population characteristics, we plotted the group-wise distributions of cell morphologies at various time points (Supplementary Figure 1). The 0 rpm control group adopts a broad distribution of cell areas within the first hour, followed by the 30 and 60 rpm groups. By 8 h, it is clear that the 0, 30, and 60 rpm cell populations encompassed comparable ranges of cell areas. The 75 rpm group, however, exhibited a much more narrow distribution. Likewise, when staining for filamentous actin we found that cells also spanned a range of cell shapes within each group (Supplementary Figure 2). There were no discernable differences in actin organization between cells of similar morphology (elongated or rounded), even when comparing across different clinorotation conditions. This suggests that the observed population differences with angular frequency is caused by disparate effects on individual cells, perhaps by triggering/overcoming some intrinsic signal within cells to reduce cell adhesion, suppress actin stress fiber formation, and consequently induce cell rounding. It is unclear whether simulated microgravity directly affects actin stress fiber assembly to result in cell rounding, or whether cell rounding induced by simulated microgravity is what inhibits stress fiber formation.

To quantify these differences in cell shape as a function of clinorotation speed, we computed circularity (circularity=4π*area/perimeter2), as it accommodates more abstract shapes than an aspect ratio calculation. We assigned circularity values above 0.6 to cells that were considered rounded (Figure 3, black), values between 0.3 and 0.6 to semi-elongated cells (Figure 3, hatch) and values below 0.3 to elongated cells (Figure 3, gray). As expected from the previous area measurements, Figure 3 clearly shows that increasing clinorotation speed results in a larger percentage of rounded cells in its population. The number of elongated cells was significantly reduced with increasing clinorotation speed, and no elongated cells were found at 75 rpm.

Figure 3
figure 3

Human mesenchymal stem cell shape as function of time at different rotation speeds. We analyzed the shapes of hMSCs at different rotation speeds as a function of time for 1, 4, and 8 h; black=rounded cells, line pattern=semi-elongated cells, gray=elongated. Cells were stained with phalloidin (actin, red) and representative micrographs were selected for each morphological configuration. At 0 rpm, cells were rounded at the first hour and were mostly elongated at the end of our time lapse. At 30 rpm, the number of elongated cells was reduced but still present at 4 and 8 h. At 60 rpm, there were no elongated cells at 4 h and there were mostly semi-elongated cells at 8 h. At 75 rpm, the number of rounded cells increases at every time point.

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Plotting cell circularity against cell area for each clinorotation speed at different time points, we clearly see a temporal increase in area associated with cell elongation in 0 rpm control cells (Supplementary Figure 3). This trend becomes disrupted with exposure to 30 and 60 rpm clinorotation, as cells tended to exhibit a broad range of circularity and area. However, only at 75 rpm the does cell population maintain high circularity and smaller areas across time points (1, 4, and 8 h). Overall, our morphology analysis demonstrates that the cell population at 75 rpm possesses a more consistent morphology (average area, cell distribution, circularity versus area over time) over time.

Cell viability and recovery after clinorotation

To determine whether there was any loss of viability or if rounded cells were undergoing apoptosis, we exposed cells to 75 rpm and used a live/dead assay after 1, 4, and 8 h of clinorotation (Figure 4b). We found no difference in cell viability or changes in cell number when compared with control; in fact, the majority of cells were alive (>90%). Under light microscopy, we observed no evidence of apoptosis (i.e., membrane blebbing) for the cells that were not viable. This also indicates that our clinochip system can be used effectively without loss of cells due to lifting or cell death for at least 8 h.

Figure 4
figure 4

Cell viability and recovery after clinorotation. (a) Cell spreading dynamics were measured for cells after 1, 4, and 8 h of clinorotation at 75 rpm. Four hours after clinorotation was terminated, cell areas were observed to increase by a factor of 1.4–1.8 times. (b) A live/dead stain was used to analyze both cells in the control and cells exposed to clinorotation, and revealed that cell viability was preserved over time. (c) A fluorescence micrograph for live cells (green) and dead cells (red) is provided to demonstrate the data we analyzed, dotted line indicates the axis of rotation. (d) Time-lapse micrographs illustrate a round cell adopting a more elongated morphology during recovery in standard microgravity.

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We investigated whether clinorotation effects on cell morphology are reversible by performing time-lapse microscopy after exposure to 1, 4, and 8 h of 75 rpm clinorotation. Following cessation of clinorotation, all cells increased their areas and round cells became more elongated, similar to most of the cells in standard gravity controls (Figure 4a). Similar experiments were also repeated for 30 and 60 rpm after 1 and 4 h of clinorotation (Supplementary Figure 4).

Simulated microgravity inhibits cell migration by inducing cell rounding

For cell migration experiments, cells were seeded in Ibidi chemotaxis chips with a chemical gradient of 100 ng/ml NGF to promote cell migration. Under clinorotation, only a few cells migrated, whereas most cells did not (see Table 2 for cell numbers). Cells that were actively migrating at 75 rpm had a similar velocity (P=0.391) and directionality (P=0.822) when compared with control cells (Figure 5). Cells that were not migrating under simulated microgravity exhibited morphological retraction (Figure 5). In other words, cell areas changed from fully spread morphologies to more rounded ones. This phenomenon is in agreement with our observations in cell-spreading experiments, even when the initial conditions were different (10 min for spreading assays versus 12 h for chemotaxis and migration assays). We found that during clinorotation cells retracted their area, but did so independently of rotation speed (‘0 h’ P=0.539, ‘1 h’ P=0.288, ‘2 h’ P=0.963, ‘3 h’ P=0.848, ‘4 h’ P=0.689, between 30 and 75 rpm). After 4 h of clinorotation during chemotaxis, cells at 30 and 75 rpm reached an average area of 2500 μm2, which is a value similar to the spreading experiments for 30 rpm at 8 h (P=0.962 between 30 rpm, P=0.975 between 75 rpm). However, we did not conduct experiments long enough to determine steady state–retracted cell areas.

Figure 5
figure 5

Analysis of chemotactic migration of human mesenchymal stem cells in simulated microgravity. Cells stimulated by a chemotactic signal (NGF) in microgravity exhibited one of two behaviors: migration or retraction. Under simulated microgravity, most cells retracted (N=17) and only some cells (N=6) actively migrated. Cells that were actively migrating (left), had a similar velocity (P=0.391) and directionality (P=0.822) in simulated microgravity to those in non-rotated conditions. Cells that did not migrate retracted their area as a function of time. This behavior was similar at different clinorotation speeds (P=0.698 at 4 h between 30 and 75 rpm). Results indicate that the morphological response to microgravity is stronger than the response to the NGF chemotactic signal. NGF, nerve growth factor.

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Our results indicate that the cellular response to simulated microgravity is more dominant than chemotactic signals, suggesting the role of migration of hMSCs to tissue repair sites might be suppressed in microgravity. We base this conclusion on our observations of response to NGF at a concentration of 100 ng/ml. However, these results were obtained with only one concentration of NGF and it is possible that different concentrations or other chemotactic molecules can elicit a stronger chemotactic response. For example stromal-derived factor-1, which is known to be a strong homing signal for hMSCs.30 Nevertheless, because the response of adhered cells to clinorotation is retraction of cellular processes, we believe that the behavior will be similar, unless the chemotactic agent can also enhance cell adhesion.

Discussion

Understanding how angular frequency, or rotation speed, of clinorotation affects cell behavior is a critical aspect of microgravity simulation experiments, so that the role of the changing gravity vector in cellular regulation can be appropriately considered. In this work we show that hMSCs can behave differently depending on clinorotation speed. In particular, although average cell area increased more slowly at 30 rpm compared with non-rotated controls, it continues along an upward trajectory at 8 h and seems to be converging with control values. For higher rotational speeds, cell area increases even more slowly, and appears to reach a plateau by 8 h at 75 rpm. This suggests that changes in cell morphology may approach a limit at an angular frequency that is close to 75 rpm, and almost certainly must exceed 30 rpm. Although these results are relevant to our clinochip configuration, results may vary for other clinostat devices, particularly for those that support cells in suspension.

Our results are consistent with other research showing that rotation speed affects animal cells, plants, and bacteria (Escherichia coli). For example, a study on osteoblastic ROS 17/2.8 cells reported that rotations at 10 and 40 rpm did not exhibit reproducible, detectable changes from stationary control cells.31 Only a speed of 50 rpm showed reproducible changes in actin cytoskeleton and cell surface integrin β1 and apoptosis. The same effect has been observed with E. coli,32 which exhibited differential response as a function of clinorotation speeds from 10 to 50 rpm. Interestingly, the difference between 40 and 50 rpm is only 0.1674 of a cycle per second, indicating that cells can be highly sensitive to small changes in angular frequency.

Although a precise gravisensing mechanism has yet to be determined, it must be one that can detect subtle alterations to external forces in a short period of time. Our data indicate that it is linked to pathways that are involved in cell spreading and cytoskeletal organization, two phenomena that have been observed for different cell types. Potential candidates could be one or more molecules already known to play important roles in cellular mechanoregulation, such as the Rho family of GTPases,33 ion mechanosensitive channels,34 intracellular calcium,35 nuclear deformations,36 focal adhesions, or other cell surface receptors.37 Although mechanosensitive pathways seem the most direct apparatus for gravisensing, others have also suggested the importance of external environmental factors including fluid shear, fluid and nutrient exchange, oxygen content, buoyancy, and changes in the extracellular matrix.38 Thus, clinostats used to probe candidate gravisensing receptors should minimize external environmental variables that arise from clinostat operation.

In the context of a proposed framework for cellular gravisensing, the current results are consistent with our working hypothetical model (Figure 1b). Standard gravity would constitute a constant gravitational stimulus and be detectable to all cells. With intermediate timescales of gravitational nullification, the probability for a single cycle of rotational perturbation to evade gravisensing in each cell would assume a broad distribution. As any putative biochemical gravisensing reaction(s) would be stochastic, the probability for gravisensory evasion in each cell would decrease with both lower angular frequency and exposure to longer duration perturbations. We did in fact observe such trends, as a result of the time lapse, single-cell measurement capabilities of the clinochip system.

For our clinochips, we do not expect that centripetal forces have a role with our observed angular frequency-dependence, as residual accelerations were calculated to be on the micro-scale regime. In addition, because the capillary number (indicative of viscous forces) is orders of magnitude smaller than surface tension, fluid shear forces are deemed negligible. There is also no enhanced nutrient transport that accompanies clinorotation in our system. Without these confounding factors, it seems reasonable to conclude that the cell morphology differences we observed were predominantly due to changes in the angular frequency of clinorotation.

We believe the rounding and retracted cell area of hMSCs in simulated microgravity inhibit migration in the presence of a chemical gradient. Interestingly, the kinetics of cell area changes during retraction were different from those during spreading, and were also angular frequency independent, suggesting that distinct gravisensing mechanisms may regulate different processes. Similarly, other cell processes, and even cell fate, could be affected.39 In the same way that microgravity may produce these cellular alterations, other mechanical stimuli and substrate characteristics can also modulate cell function.40

Stem cell morphology has a strong correlation with cellular phenotype and differentiation potential.41,42 It has been demonstrated in prior work that spread cells have a higher tendency to undergo osteogenesis and that cells with rounded morphologies are more susceptible to adipogenesis.42 Because of the short-term nature of this current study, it is not possible to establish whether hMSCs in our system would behave according to these trends. However, our data would suggest that cells at 30 rpm clinorotation would be more amenable to osteogenic differentiation, whereas cells at 75 rpm would tend toward adipogenic or chondrogenic lineages. This may help explain the conflicting reports on mesenchymal stem cells differentiation during clinorotation that we and others23 have observed. Future longer-term studies with the clinochip are required to explore hMSC differentiation potential. Specifically, as we have shown that the population distribution of cell morphologies can be controlled by the angular frequency of rotation, we may be able to derive cellular phenotypes desirable for stem cell renewal, repair, and tissue engineering.