Fluid pressure in human dermal fibroblast aggregates measured with micropipettes

L. E. B. Stuhr,1 A. Reith,1 S. Lepsøe,1 R. Myklebust,2 H. Wiig,1 and R. K. Reed1

1Department of Physiology and 2Department of Anatomy and Cell Biology, University of Bergen, N-5009 Bergen, Norway

Submitted 5 February 2003 ; accepted in final form 2 July 2003


    ABSTRACT
 TOP
 ABSTRACT
 METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Previous studies indicated that connective tissue cells in dermis are involved in control of interstitial fluid pressure (Pif). We wanted to develop and characterize an in vitro model representative of loose connective tissue to study dynamic changes in fluid pressure (Pf) over a time course of a few minutes. Pf was measured with micropipettes in human dermal fibroblast cell aggregates of varying size (<100- and >100-µm diameter) and age (days 1-4) kept at different temperatures (~15, 25, and 35°C). Pressures were measured at different depths of micropipette penetration and after treatment with prostaglandin E1 isopropyl ester (PGE1), latanoprost (PGF2{alpha}), and ouabain. Pf was positive (more than +2 mmHg) during control conditions and increased with increasing aggregate size (day 2), age (day 4 vs. day 1), temperature, and depth of micropipette penetration. Pf decreased from 2.9 to 2.0 mmHg during the first 10 min after application of 10 µl of 1 mM PGE1 (P < 0.001). Pf increased from 3.0 to 4.8 mmHg (P < 0.01) after administration of 10 µl of 1.4 µM ouabain and from 3.1 to 4.4 mmHg after addition of 5 µl of 1.42 mM PGF2{alpha} (P > 0.05). In conclusion, we have developed and validated a new in vitro method for studying fluid pressure in loose connective tissue elements with the advantage of allowing reliable and rapid screening of substances that have a potential to modify Pf and studying in more detail specific cell types involved in control of Pf. This study also provides evidence that fibroblasts in the connective tissue can actively modulate Pf.

micropuncture; prostaglandin E1; prostaglandin F2{alpha}; ouabain; integrins


INTERSTITIAL FLUID PRESSURE (Pif) is one of the determinants of transcapillary fluid exchange and plays an important role in controlling interstitial fluid volume (24). In previous studies Pif was measured in different animal tissues with micropuncture after the administration of test substances either locally or systemically (24). Pif in skin is normally approximately -1 mmHg (36), whereas during burn injury and inflammation Pif is lowered substantially and hence becomes an important contributor to increasing capillary filtration and edema formation (17, 18, 25). The mechanisms that generate such changes in Pif are presently not fully understood.

During recent years our group has demonstrated that the cells of the connective tissue can influence the physical properties of the extracellular matrix. They actively participate in transcapillary fluid exchange by altering Pif and hence play an important role in controlling interstitial fluid volume (24). Meyer (19) showed that connective tissue, when allowed free access to fluid, swelled because of its content of glycosaminoglycans and hyaluronan. This tissue swelling was counteracted by the collagen and microfibril networks. Dermal fibroblasts cultured in three-dimensional collagen gels contract the gel (1, 2, 20), indicating that the connective tissue cells exert tensile forces. The contraction has been shown to be dependent on the collagen-binding {beta}1-integrin, one of eight subfamilies of {beta}-integrins (10, 11, 15, 26, 29).

Fibroblasts are the predominant cell type in the connective tissue. They are responsible for synthesis of collagen, elastic fibers, and the complex carbohydrates of the connective tissue (12). The fibroblast cells within an aggregate are held together by cell processes, cell adhesion molecules, extracellular matrix proteins, and a variety of cell-cell junctions (32).

The most commonly used in vitro system used to study cell-matrix interaction is the collagen gel contraction assay, in which ~100,000 fibroblasts are mixed with {alpha}-helical collagen. Within 24 h the fibroblast compacts the gel to ~10% of its original volume. Agents that act on the cell-matrix contact or the rate of compaction raise or slow the rate of compaction with an effect that is detectable in the course of hours. The aim of this study was therefore to develop, and thereafter characterize, an in vitro model of loose connective tissue using human dermal fibroblast cell aggregates to study the dynamic changes in pressure in the aggregates over a time course of a few minutes.


    METHODS
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 ABSTRACT
 METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Preparation of Human Dermal Fibroblasts

Human skin (5 x 5 cm) was obtained from patients undergoing plastic surgery for stomach reduction. The patients gave their informed consent, and approval of the study was given by the Regional Ethical Committee. The skin was washed in sterile phosphate-buffered saline (PBS) and transferred to a sterile petri dish, where the subcutaneous fat was removed by dissection. Thereafter, the skin was cut into very fine pieces (<1 mm2) and suspended in a minimal amount of Dulbecco's modified Eagle's medium (DMEM; PAA Laboratories, Linz, Austria). This medium was supplemented with 10% fetal calf serum (FCS), 100 U/ml penicillin, 100 µg/ml streptomycin, and 1% L-glutamine (Life Technologies, Paisley, UK) and seeded in a 75-cm2 tissue culture flask (Nunc, Nalga Nunc International). The tissue explants were cultured without disturbance until fibroblast cell outgrowth was detected. The medium was replenished at this stage, and the cells were subcultured when significant cell growth was observed and grown to confluence. Primary cultures of fibroblasts between passages 1 and 8 were used. All cells were cultured under standard conditions at 37°C in a humidified atmosphere of 5% CO2-95% air.

Preparation of Cell Aggregates

Cell aggregates were prepared with human dermal fibroblasts at passages 2-8. Three-dimensional aggregates were prepared according to the method of Yuhas et al. (34). Cell culture flasks (25 cm2) were base coated with 0.75% agar in 5 ml of DMEM. Fibroblasts were seeded at a density of 3 x 106 cells per 25-cm2 flask. The cells were cultured without disturbance until the cell aggregates formed.

Transmission Electron Microscopy

Human dermal fibroblast cell aggregates were cultured, carefully placed in a test tube, and fixed in 2% glutaraldehyde in 0.2 M cacodylate buffer (pH 7.2). They were rinsed in 0.1 M cacodylate buffer (2 x 15 min), postfixed in 1% osmium tetroxide for 35 min, and dehydrated in a series of ascending concentration gradients of ethanol. Specimens were then embedded in araldite plastic. The semithin sections were stained with 1% toluidine blue. The ultrathin sections were double stained with 1% uranyl acetate (20 min) and lead citrate (10 min) before being viewed in a JEOL 100CX transmission electron microscope.

Measurement of Fluid Pressure

Fluid pressure (Pf) in the three-dimensional cell aggregates was measured with a micropuncture system. A borosilicate glass pipette (GC 100-15, 1-mm OD x 0.58-mm ID) was pulled on a micropipette puller (P-87; Sutter Instruments). The tip was sharpened to a diameter of 3-9 µm. The pipette was filled with 0.5 M NaCl solution colored with Evans blue dye. The pipette was then connected to a micromanipulator (Leitz) and a servo-controlled counterpressure system (36). Calibration was performed before each experiment. Zero control pressure was measured in a bath of 0.9% NaCl (isotonic saline) that was set at the same height as the petri dish containing the cell aggregates to be micropunctured. Measurements of aggregate pressure (Pf) were performed by inserting the glass pipette directly into the central part of the fibroblast aggregate with the use of a stereomicroscope (Wild M5, Heerbrugg, Switzerland). There was no visible compression or retraction of the aggregate during the micropuncture procedure. Only aggregates that were attached to the bottom of the petri dish could be micropunctured. The following criteria had to be fulfilled for the measurements to be accepted: 1) The recorded pressure did not change when the feedback gain of the servo-controlled unit was varied. 2) After fulfillment of the first criterion, communication between the fluid in the pipette and the fibroblast cell fluid was tested by applying suction to the pipette, which should raise electrical resistance in the pipette because of the entry of fluid with a low tonicity. 3) The zero pressure measured in the bath of saline after micropuncture returned to the initial zero measurement.

Measurements

Unless otherwise stated, the measurements were performed under control conditions, defined as a medium temperature >20-24°C, cell aggregates of passages 7-8, and measurements performed in the central part of the aggregate. We have not been able to demonstrate any cell characteristics differences between passages 7 and 8 in our study. Aggregate Pf was also measured under the conditions described below.

Cell aggregates of different sizes. Cell aggregates <100 and >100 µm in diameter were used. The aggregate size was measured with an eyepiece graticule (Mol-93; Leica).

Cell aggregates of different ages. Aggregates were cultured and kept under standard culture conditions at 37°C in a humidified atmosphere and measured on day 1, 2, 3, or 4 to see whether age influenced Pf.

Different depths of penetration within the cell aggregate. To relate Pf to depth of penetration within the cell aggregate, long pipette advancement distances were required and pipettes were made with a long shank to minimize tissue distortion and compression artifacts at deep insertion distances. A dial indicator was mounted onto the fixed part of the micromanipulator, allowing measurement of the pipette advancement to the nearest 10 µm. With the pipette on the aggregate surface, the angle over the horizontal plane between aggregate and pipette was measured to the nearest degree and the pipette was inserted. The depth of measurement was then calculated as the distance of advancement times the sine of the angle between the horizontal plane and pipette. Three or four pressure measurements were recorded within each cell aggregate during the insertion from the surface to the center, with each recording lasting 1-3 min.

Different temperatures. The cells were taken directly from the 37°C culture incubator to the laboratory. At room temperature the bath temperature was measured at 25°C. The petri dish was placed on a bed of ice for measurements at 15°C. Measurements performed at 35°C required the petri dish to be placed on a heating plate set at 35°C. The medium temperature was monitored in the petri dish throughout the experiment with a digital thermometer. It was assumed that the temperature within the aggregate was the same as that in the surrounding medium.

Under influence of test drugs. A 2-min stable Pf control period was always obtained before measurements commenced. The drugs were dropped carefully onto the fibroblast cell aggregate, and the effect was studied over a period of 20-30 min. All measurements in this group were performed at room temperature, and only one aggregate was measured in each petri dish. To evaluate a possible effect of the application procedure, a control study using 10 µl of saline (0.9% NaCl; n = 3) was performed. Prostaglandin E1 isopropyl ester (PGE1; n = 10) was obtained from Sigma (St. Louis, MO). PGE1 is a nonselective prostanoid EP receptor agonist and was applied at 1 mM in a volume of 10 µl. PGF2{alpha} (latanoprost, lithium salt; n = 10) was obtained from Sigma. Latanoprost is a selective prostanoid FP receptor agonist and was applied at 1.42 mM in a volume of 5 µl. Ouabain (n = 10) was also obtained from Sigma. Ouabain is a Na+-K+-ATPase inhibitor and was applied at 1.4 µM in a volume of 10 µl.

Statistical Analysis

One-way analysis of variance (ANOVA) with repeated measurements followed by Bonferroni's test was used for statistical analysis. P < 0.05 was considered statistically significant. Data are given as means ± SD.


    RESULTS
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 METHODS
 RESULTS
 DISCUSSION
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Transmission Electron Microscopy

The cell aggregate ultrastructure is shown in Figs. 1 and 2. Figure 1 (semithin section) shows that the cell aggregate is cohesive and almost spherical in form. The cell aggregates ranged from ~40 to 350 µm in diameter. Figure 2 (ultrathin section) shows that the cell aggregate was comprised of numerous fibroblast cells with many vacuoles and nuclei and endoplasmic reticulum. The intercellular spaces were frequently filled with collagenous, fibrillar, and amorphous material. The fibroblasts were connected by scattered junctions as seen in Fig. 2. A distinct extracellular basal membrane was not observed.



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Fig. 1. Transmission electron microscopy of a human dermal fibroblast cell aggregate (semithin section).

 


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Fig. 2. Transmission electron microscopy of a human dermal fibroblast cell aggregate magnified x5,000 (ultrathin section). Cell junctions are marked with arrows.

 

Control Pf (n = 33)

The fibroblast cell aggregate Pf was always positive and relatively high (more than +2 mmHg) during control conditions, with an average of 3.1 ± 0.8 mmHg.

Effect of Size on Pf (n = 47)

There was a tendency for larger aggregates (>100 µm) to have a higher Pf than small aggregates (<100 µm). The difference in Pf related to size was statistically significant only at day 2 vs. day 1 (P < 0.01) (Fig. 3). The average Pf was 4.6 and 2.5 mmHg in large and small aggregates, respectively, at day 2.



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Fig. 3. Effect of human dermal fibroblast aggregate size (small: <100 µm, large: >100 µm) and age (days 1-4) on fluid pressure (Pf). Values are means ± SE. **P > 0.01 large vs. small aggregates, ##P < 0.01 vs. day 1 (small aggregates).

 

Effect of Age on Pf (n = 47)

Cell aggregates were studied over a 4-day period. There was a statistically significant effect of age on Pf (P < 0.01), i.e., passage number, at day 4 vs. day 1 in small aggregates (Fig. 3). The average Pf was 2.5 mmHg at day 1 compared with 3.8 mmHg at day 4 in the small aggregates.

Effect of Depth on Pf (n = 36)

A significant increase in Pf was found toward the center of the fibroblast cell aggregate (Fig. 4). The average Pf was 2.4 mmHg just under the surface and 4.6 mmHg in the center of the aggregate.



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Fig. 4. Aggregate Pf relative to depth (0 = surface, 1.0 = center). Values are means ± SE. **P > 0.01 vs. superficial layer (0.2).

 

Effect of Temperature on Pf (n = 46)

Increasing temperature significantly raised Pf (Table 1). The difference between the three temperature groups was statistically significant (P < 0.01). To eliminate external factors, all the aggregate groups had a similar average size and were taken from the same passages (7 and 8) and measurements were made in the center of the aggregate.


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Table 1. Effect of temperature on fluid pressure in dermal fibroblasts

 

Effects of Saline, PGE1, Ouabain, and Latanoprost

The effects of saline, PGE1, ouabain, and latanoprost on aggregate Pf over a period of 20-30 min are shown in Fig. 5. There was no effect on Pf when 10 µl of saline (n = 3) was applied in an identical way as the test substances to the aggregates. Before the administration of PGE1 (n = 10), control Pf averaged 2.9 mmHg. Pf started to decrease immediately after 10 µl of PGE1 was applied. After 10 min, the Pf was ~2.0 mmHg and it then started to increase again (Fig. 5A). Before treatment with PGF2{alpha} (n = 10), control Pf was 3.1 mmHg and increased rapidly after 5 µl of latanoprost were applied until it stabilized at 4-5 mmHg. It maintained this value for the following 6-20 min (Fig. 5B). Before treatment with ouabain (n = 10), control Pf averaged 3.0 mmHg. As for PGF2{alpha}, pressure started to increase after the application of 10 µl of ouabain (Fig. 5C). Ten minutes after application Pf averaged 4.8 mmHg, whereas Pf returned to control values after 20 min.



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Fig. 5. Effects of prostaglandin (PG)E1 (1 mM, 10 µl; A), PGF2{alpha} (latanoprost; 1.42 mM, 5 µl; B), and ouabain (1.4 µM, 10 µl; C) on aggregate Pf over a period of 20-30 min. The drug was applied immediately after control measurements (0 min). Values are means ± SE. *P < 0.05, **P < 0.01, ***P < 0.001 vs. control.

 


    DISCUSSION
 TOP
 ABSTRACT
 METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
In the present study we have demonstrated that human dermal fibroblast aggregates can be used as an effective in vitro model for loose connective tissue. Anchorage-dependent cells, having cell adhesion molecules on the surface, have the ability to form cell clusters or aggregates if the seeding density is sufficiently high. Fibroblast cells formed spherical aggregates (Fig. 1). In monolayer cultures, the cells become grossly elongated and distorted when they adhere to the plastic substratum of the culture flask. The present cells maintain the size and ultrastructure that they possess in the skin. Cells cultured as spherical aggregates form cell junctions (34), possess cell adhesion molecules, and have the ability to synthesize proteins (4) and form cell adhesion and junctions (34) similar to those found in the tissue of origin. In parallel with keratinocytes in skin (28, 37) and fibroblast-populated collagen lattices (7), the fibroblast aggregates used in the present study demonstrated tight junctions, suggesting that cell-cell communication might take place. However, no attempt was made, for example, by using Lucifer yellow, to demonstrate whether this actually was the case. Nevertheless, the demonstration of tight junctions suggests that the fibroblasts still maintained their ability to form cell-cell communication. We therefore believe that these aggregates are a good in vitro model for mimicking the interstitium.

Pressure in the human dermal fibroblast cell aggregates (Pf) was measured with a micropuncture method previously used to measure Pif in vivo in mice, rats, cats, and dogs (24). The only practical consideration when measuring Pf in an aggregate is that it must be anchored to the petri dish, because the pipette could not otherwise be advanced into the aggregate because of aggregate movement. Otherwise, the micropuncture method was used as in previous in vivo studies.

The primary aim of this study was to establish and characterize an in vitro model to study dynamic changes in cell-matrix interactions through the response on Pf as an alternative to using collagen gel contraction assays. The collagen gel contraction assay is based on the ability of fibroblast cells to organize and compact a collagen lattice. Briefly, ~100,000 fibroblasts are mixed with soluble type I collagen. The fibroblast cells contract the collagen fibers to between 10% and 20% of their starting volume within 24 h (14, 33). The contraction is mediated via heterodimeric {beta}1-integrin cell-matrix receptors. The rate of gel contraction is dependent on several factors, including the type and number of cell-matrix attachments as well as the cytoskeleton to which the integrins are attached. Cytokines and chemokines influence the affinity and avidity of the integrins and can therefore exert an effect on the rate of contraction of the collagen gel in the contraction assay. Agents that influence the speed of contraction will either enhance or diminish the rate of contraction, but usually several hours are required to detect a response. The primary aim of the present study was to develop a method with a more rapid response than can be obtained with the collagen gel contraction assay. It was also important that the in vitro model described in this study gives a response to compaction or expansion of the aggregate in opposite directions. In this respect it differs from the collagen gel contraction assay, in which, although there are different rates of response, contraction forces are measured in one direction. The aims of this study were accomplished in that the cell aggregate system responded rapidly (within 1-2 min) and consistently in both positive and negative directions to the pharmacological agents applied. Pf in the control was positive, and the response to PGE1 was in agreement with the in vivo response observed previously (2).

To the best of our knowledge Pf has not been measured previously in human dermal fibroblast cell aggregates, and the observations reported here allow suggestions as to the mechanisms that generate and influence Pf. To more fully explain the model, we also discuss parallel observations in vivo and in other experiments. Under control conditions, Pf in normal fibroblast cell aggregates was >=2 mmHg. The most likely explanation for the positive pressure relative to the ambient fluid in the aggregates would appear to be that water is transported into the central part of the aggregate by active cellular transport and then transported by convection from the interior of the aggregate into the surrounding medium. In addition, there are tensile forces generated by the fibroblast that would also appear to contribute to the normal balance of forces in the normal steady state. These suggestions are founded on the observation that Pf fell and increased in parallel with a lowering or raising temperature, i.e., Pf is dependent on processes requiring energy. Several studies have recently quantified the force produced by single cells (35), although the size of the force measured varied according to the method used. Fibroblast-populated collagen gel lattice (FPCL) studies and the use of force transducers measured a force of 0.1-2 nN per cell (3, 5). Contractile forces, generated by single fibroblast cells with elastomer sheets, demonstrated 2.0 µN per cell (33), an ~1,000-fold higher value than the FPCL studies. Because the FPCL method measures force and stiffness of whole populations, the difference is probably due to this. There is, however, a general agreement that human dermal fibroblasts can generate tension. The {alpha}-actin filaments in human dermal fibroblasts can produce force (38). The force generated by actin microfilaments is transmitted from a cell to the extracellular matrix via the integrin receptors (6, 35). As shown in this study, human fibroblast cells are in contact through junctions, thus contributing a cellular network, which is important in the transmission of contact throughout the aggregate.

Adhesion properties and expression of extracellular matrix receptors bind the fibroblast cells together as well as to the extracellular matrix, but they differ among different fibroblast populations (23). Integrins constitute a large family of adhesion receptors. The {beta}1-integrins have an important role in tension generation in dermal fibroblasts by mediating the force generated from the cytoskeleton through the cell membrane via the integrins and on to the extracellular matrix. This was shown in dermal fibroblasts embedded in the collagen gel, when force generation was effectively inhibited with antibodies that reversibly blocked ligand binding via the {beta}1-integrins and the extracellular matrix (10, 14, 15, 26, 29).

The model, which is visualized for the cellular control of Pif, is based on in vitro experiments by Meyer (19) as well as our own experiments. Umbilical cord, which is a typical loose connective tissue, will double its volume in 24-48 h when placed in saline. The swelling property is generated by the tissue's content of hyaluronan and glycosaminoglycans. At the same time, the swelling is restrained by microfilament and collagen networks within the tissue because enzymatic degradation of these networks enhances the swelling. Perturbation of {beta}1-integrin function with monoclonal antibodies to this receptor, or monoclonal antibodies to the {alpha}2{beta}1-integrin, induces lowering of Pif concomitant with edema formation (26, 27). A series of parallel in vivo and in vitro experiments have demonstrated similar responses in that the agents that reduce the speed of contraction in the collagen gel contraction lattice induce a lowering of Pif, whereas agents that enhance the rate of contraction reverse a lowering of Pif. In light of these observations and those of Meyer (19), the model that is used to describe the cellular effects in control of Pif is as follows: the perturbation of the cell-matrix contact will reduce the tension mediated from cells on the fiber networks and allow the tissue to swell because of hyaluronan and glycosaminoglycan content. When no fluid is available to enter the tissue initially Pif will fall until a new balance is reached between the lowered Pif, the ability to swell, and the stress in the filament networks induced by the cellular tension and their inherent biochemical properties. The lowered Pif will move water from capillaries and subsequently raise Pif toward and above control values again until a new steady state is reached between Pif, the swelling properties, and the stress in the fiber networks.

The second aim of this study was to elucidate whether the aggregates respond to pharmacological agents previously demonstrated to have an effect on Pif in vivo and the collagen gel contraction assay that led to the model described above. Application of PGE1 to the aggregates induced a rapid fall in Pf. PGE1 binds to prostanoid receptors of the EP type and prostacyclin receptors (IP) (21), suggesting that the normal tensile forces within the fibroblasts would be reduced by loosing or diminishing their attachments. The lowering of Pf after PGE1 is in parallel to the effect on Pif when PGE1 is injected in vivo (2) and a reduction in the collagen gel contraction rate (2). This also corresponds to previous studies using PGE1 and interleukin-1, which showed inhibition of fibroblast-mediated collagen gel contraction (2, 8, 9, 33).

With the application of latanoprost, a PGF2{alpha} analog and selective prostanoid FP receptor agonist, the effect was opposite to that of PGE1. Latanoprost was previously shown to reverse the decrease observed in Pif during inflammation, although it had no effect on Pif by itself (2). Binding of latanoprost to the FP and {beta}1-integrin receptors was probably the reason for contraction of the fibroblasts and thus the enhanced Pf.

Because of the effects of PGE1 and PGF2{alpha}, prostanoid receptors EP, IP, and FP must be expressed on the human dermal fibroblast cells. The affinity and avidity of the {beta}1-integrins in the fibroblast aggregates are also most likely modulated by prostaglandins, allowing for rapid changes in the balance between grip and release.

Ouabain, which is a well-known Na+-K+-ATPase inhibitor, raised Pf in the fibroblast aggregates. The response was in the expected direction because inhibition of Na+-K+-ATPase will cause the individual cell to swell, in turn raising Pf.

Together, these experiments demonstrate that Pf is influenced by two individual processes: first, the cell-matrix interaction, as demonstrated by the effects of PGE1 and PGF2{alpha}, and second, cell volume, as demonstrated by the use of ouabain causing cell swelling and increased Pf. The effect of temperature is likely due to a combination of two processes, a diminished contraction of the cells in the aggregates on the matrix (31) and cell swelling caused by diminished pumping activity of the Na+-K+-ATPase (13, 16). Both the Na+-K+-ATPase- and the cytoskeleton-induced compaction on the matrix are energy-dependent processes. This effect is similar to ouabain with reduced pumping activity because the Na+-K+-ATPase is an energy-dependent process. Energy-dependent processes in general are reduced by 50% for every 10°C lowering of temperature. However, the overall effect of cooling was opposite to that of ouabain, and therefore other processes must also be involved. The effect of PGE1 is to diminish the cell matrix, which is in parallel with the observation that lowering the temperature will lower the cytoskeleton-induced contraction in collagen gels (22, 30) and in isolated neonatal rat myocardial cells (30). The observations that the two energy-requiring processes of Na+-K+-ATPase- and cytoskeleton-induced contraction affect Pf in opposite directions, combined with the fact that the overall effect of lowering temperature decreases Pf, strongly suggest that cytoskeletal relaxation is overriding the effect of Na+-K+-ATPase on Pf.

Although the pressure in the aggregates is positive, the responses to pharmacological agents are in a direction and of a magnitude similar to those observed in vivo. Although the response is more short-lasting than in vivo (about half that seen in vivo), it is nevertheless of a magnitude similar to that seen in vivo. This is possibly caused by the excess of free fluid surrounding the aggregates ("washing" out the pharmacological agents quickly), which is not the case for skin and dermis in vivo.

Thus the aggregates respond in a manner that is in parallel to the in vivo situation as well as the collagen gel contraction assay. This would then confirm the model for control of interstitial fluid pressure developed based on these systems. The spheroids have a time response and magnitude and direction of the pressure response very similar to those seen in vivo. This will allow for rapid screening of substances for in vivo use, as well as for an improved understanding of which connective tissue cells participate in control of interstitial pressure.

In conclusion, we have developed cellular aggregates that can be used to study dynamic interactions in the connective tissue and are an effective alternative to the collagen gel contraction assay. Cytoskeletal contraction, cell volume regulation, and cell-matrix interactions influence Pf as demonstrated in the present experiments. A positive Pf was observed with increasing size, age, measured depth, and temperature. The human dermal fibroblast cell aggregates provide rapid responses (within minutes) in a more positive or negative direction. Finally, the present study provides evidence for the active modulation of fluid pressure via fibroblasts in the connective tissue.


    DISCLOSURES
 
Financial support was obtained from The Norwegian Research Council and The Norwegian Heart Association. A. Reith was partly funded by European Union Training and Mobility of Researchers Grant ERBFMRXCT980219.


    FOOTNOTES
 

Address for reprint requests and other correspondence: L. E. B. Stuhr, Dept. of Physiology, Univ. of Bergen, Jonas Liesv. 91, N-5009 Bergen (E-mail: linda.stuhr{at}fys.uib.no).

The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.


    REFERENCES
 TOP
 ABSTRACT
 METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
1. Bell E, Ivarsson B, and Merrill C. Production of tissue-like structure by contraction of collagen lattices by human fibroblasts of different proliferative potential in vitro. Proc Natl Acad Sci USA 79: 1274-1278, 1979.

2. Berg A, Ekwall AKH, Rubin K, Stjernschantz J, and Reed RK. Effect of PGE1, PGI2, and PGF2{alpha} analogs on collagen gel compaction in vitro and interstitial pressure in vivo. Am J Physiol Heart Circ Physiol 274: H663-H671, 1998.[Abstract/Free Full Text]

3. Brown RA, Prajapati R, McGrouther DA, Yannas IV, and Eastwood M. Tensional homeostasis in dermal fibroblasts: mechanical responses to mechanical loading in three-dimensional substrates. J Cell Physiol 175: 323-332, 1998.[ISI][Medline]

4. Durand RE and Sutherland RW. Effects of intracellular contact on repair of radiation damage. Exp Cell Res 71: 75-86, 1972.[ISI][Medline]

5. Eastwood M, McGrouther DA, and Brown RA. A culture force monitor for measurement of contraction forces generated in human dermal fibroblast cultures: evidence for cell-matrix mechanical signalling. Biochim Biophys Acta 1201: 186-192, 1994.[ISI][Medline]

6. Elson EL. Cellular mechanics as an indicator of cytoskeletal structure and function. Annu Rev Biophys Biophys Chem 17: 397-430, 1988.[ISI][Medline]

7. Erhlich HP, Gabbiani G, and Meda P. Cell coupling modulates the contraction of fibroblast-populated collagen lattices. J Cell Physiol 184: 86-92, 2000.[ISI][Medline]

8. Erhlich HP, Rockwell WB, Cornwell TL, and Rajarathnam JB. Demonstration of a direct role for myosin light chain kinase in fibroblast-populated collagen lattice contraction. J Cell Physiol 146: 1-7, 1991.[ISI][Medline]

9. Gillery P, Cousty F, Pujol JP, and Borel JP. Inhibition of collagen synthesis by interleukin-1 in three-dimensional collagen lattice cultures of fibroblasts. Experientia 45: 98-101, 1989.[ISI][Medline]

10. Gullberg D, Tingstøm A, Thuresson AC, Olsson L, Terracio L, Borg TK, and Tubin K. {beta}1-integrin-mediated collagen gel contraction by PDGF. Exp Cell Res 186: 264-272, 1990.[ISI][Medline]

11. Gullberg D, Turner DC, Borg TK, Terracio L, and Tubin K. Different {beta}1-integrin collagen receptors on rat hepatocytes and cardiac fibroblasts. Exp Cell Res 190: 254-264, 1990.[ISI][Medline]

12. Hashimoto K. Normal and abnormal connective tissue of the human skin. I. Fibroblast and collagen. Int J Dermatol 17: 459-471, 1978.[ISI][Medline]

13. Honig A, Oppermann H, Budweg C, Goldbecher H, and Freyse EJ. Demonstration of temperature dependence of Na+-K+ pump activity of human blood cells. Am J Physiol 266: S10-S15, 1994.[Medline]

14. Jenkins G, Redwood KL, Meadows L, and Green MR. Effect of gel re-organization and tensional forces on the {alpha}2{beta}1 integrin levels in dermal fibroblasts. Eur J Biochem 263: 93-103, 1999.[Abstract/Free Full Text]

15. Klein CE, Dressel D, Steinmayer T, Mauch C, Eckes B, Krieg T, Bankert RB, and Weber L. Integrin {alpha}2{beta}1 is upregulated in fibroblasts and highly aggressive melanoma cells in three-dimensional collagen lattices and mediates the reorganization of collagen I fibrils. J Cell Biol 115: 1427-1436, 1991.[Abstract]

16. Larsen T, Solberg S, Johansen R, and Jørgensen L. Effect of cooling on the intracellular concentration of Na+, K+, and Cl- in cultured human endothelial cells. Scand J Clin Lab Invest 48: 565-571, 1988.[ISI][Medline]

17. Lund T, Onarheim H, Wiig H, and Reed RK. Mechanisms behind increased dermal imbibition pressure in acute burn edema. Am J Physiol Heart Circ Physiol 256: H940-H948, 1989.[Abstract/Free Full Text]

18. Lund T, Wiig H, and Reed RK. Acute postburn edema: role of strongly negative interstitial fluid pressure. Am J Physiol Heart Circ Physiol 255: H1069-H1074, 1988.[Abstract/Free Full Text]

19. Meyer FA. Macromolecular basis of glomerular protein exclusion in loose connective tissue and of swelling pressure (umbilical cord). Biochim Biophys Acta 755: 388-399, 1983.[ISI][Medline]

20. Nakagawa S, Pawelek P, and Grinnell F. Extracellular matrix organization modulates fibroblast growth and growth factor responsiveness. Exp Cell Res 182: 572-582, 1989.[ISI][Medline]

21. Negishi M, Sugimoto Y, and Ichikawa A. Molecular mechanisms of diverse actions of prostanoid receptors. Biochim Biophys Acta 1259: 109-119, 1995.[ISI][Medline]

22. Nishiyama T, Tominaga N, Nakajima K, and Hayashi T. Quantitative evaluation of the factors affecting the process of fibroblast-mediated collagen gel contraction by separating the process into three phases. Coll Relat Res 8: 259-273, 1988.[ISI][Medline]

23. Palaiologou AA, Yukna RA, Moses R, and Lallier TE. Gingival, dermal, and periodontal ligament fibroblasts express different extracellular matrix receptors. J Periodontol 72: 798-807, 2001.[ISI][Medline]

24. Reed RK. Interstitial fluid pressure. In: Interstitium, Connective Tissue and Lymphatics, edited by McHale N, Bert JL, Winlove P, and Lane GA. London, UK: Portland, 1995, p. 85-100.

25. Reed RK and Rodt SÅ. Increased negativity of interstitial fluid pressure during the onset stage of inflammatory edema in rat skin. Am J Physiol Heart Circ Physiol 260: H1985-H1991, 1991.[Abstract/Free Full Text]

26. Reed RK, Rubin K, Wiig H, and Rodt SÅ. Blockade of {beta}1-integrins in skin causes edema through lowering of interstitial fluid pressure. Circ Res 71: 978-983, 1992.[Abstract]

27. Rodt SÅ, Åhlen K, Berg A, Rubin K, and Reed RK. A novel physiological function for platelet-derived growth factor-BB in rat dermis. J Physiol 495: 193-200, 1996.[Abstract]

28. Salomon D, Saurat JH, and Meda P. Cell-to-cell communication within intact human skin. J Clin Invest 82: 248-254, 1988.[ISI][Medline]

29. Schiro JA, Chan BMC, Roswit WT, Kassner PD, Pentland AP, Hemler ME, Eisen AZ, and Kupper TS. Integrin {alpha}2{beta}1 (VLA-2) mediates reorganization and contraction of collagen matrices by human cells. Cell 67: 403-410, 1991.[ISI][Medline]

30. Souren JEM, Schneijdenberg C, Verkleij AJ, and Van Wijk R. Factors controlling the rhythmic contraction of collagen gels by neonatal heart cells. In Vitro Cell Dev Biol 28: 199-204, 1992.

31. Steinberg BM, Smith K, Colozzo M, and Pollack R. Establishment and transformation diminish the ability of fibroblasts to contract a native collagen gel. J Cell Biol 87: 304-308, 1980.[Abstract]

32. Sutherland RM. Cell and environment interactions in tumor microregions: the multicell spheroid model. Science 8: 177-184, 1988.

33. Tingstrøm A, Heldin CH, and Rubin K. Regulation of fibroblast-mediated collagen gel contraction by platelet-derived growth factor, interleukin-1 and transforming growth factor-beta 1. J Cell Sci 102: 315-322, 1992.[Abstract]

34. Yuhas JM, Li AP, Martinez AO, and Ladman AJ. A simplified method for production and growth of multicellular tumor spheroids. Cancer Res 37: 3639-3643, 1977.[Abstract]

35. Wakatsuki T, Schwab B, Thompson C, and Elson EL. Effects of cytochasin D and latrunculin B on mechanical properties of cells. J Cell Sci 114: 1025-1036, 2000.[ISI]

36. Wiig H, Reed RK, and Aukland K. Micropuncture measurement of interstitial fluid pressure in rat subcutis and skeletal muscle: comparison to wick-in-needle technique. Microvasc Res 21: 308-319, 1981.[ISI][Medline]

37. Wiszniewski L, Limat A, Saurat JH, Meda P, and Salomon D. Differential expression of connexins during stratification of human keratinocytes. J Invest Dermatol 115: 278-285, 2000.[ISI][Medline]

38. Wrobel LK, Fray TR, Molloy JE, Adams JJ, Armitage MP, and Sparrow JC. Contractility of single human dermal myofibroblasts and fibroblasts. Cell Motil Cytoskeleton 52: 82-90, 2002.[ISI][Medline]





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