Could radial extracorporeal shock wave therapy have an effect on wound healing in clinical practice by creating genotoxic damage? An in vitro study in mouse fibroblasts
1Department of Orthopedics and Traumatology, Başkent University, Faculty of Medicine, Ankara, Turkey
2Department of Medical Biology, Başkent University, Faculty of Medicine, Ankara, Turkey
3Department of Medical Biology, Kırıkkale University, Faculty of Medicine, Kırıkkale, Turkey
Keywords: Cell viability, extracorporeal shock wave therapy, genotoxicity, in vitro, wound healing
Objectives: This study aims to evaluate wound healing effects of in vitro radial extracorporeal shock wave (rESW) application on mouse fibroblasts and whether the cytotoxic effect of extracorporeal shock wave (ESW) was due to a possible genotoxic effect.
Patients and methods: After creating an in vitro wound healing model in L929 mouse fibroblast culture, fibroblasts were stimulated with a frequency of 3 Hz, and 100, 250, 500, 1,000 and 1,500 pulses shock waves were applied. Energy flux densities ranging from 0.01 to 0.23 mJ/mm2 (14.3 MPa) at a constant pressure level of 0.5 and 1 bar were applied. Wound healing, cell viability, and genotoxicity were evaluated at 24 and 48 h.
Results: All shot numbers for both pressures significantly reduced cell viability (p<0.05). For both 0.5 and 1 bar pressures, in both intervals, the rate of wound healing decreased, regardless of the number of shots (p<0.05). In vitro genotoxic damage was detected at both 0.5 and 1 bar pressures, in both time intervals, regardless of the number of shots. The genotoxic damage increased from 24 to 48 h.
Conclusion: The study results suggest that, when ESWT is applied in this in vitro experimental setup, cell viability decreases and wound healing is delayed under all conditions. Furthermore, genotoxic damage can be prevented by using shots below 1,000 pulses. Therefore, while investigating the therapeutic effect of ESW therapy in vitro, the upper limit for the number of shots should be 1,000 pulses.
Extracorporeal shock wave therapy (ESWT) is a noninvasive treatment method using sound waves to stimulate healing. The number of studies in the literature has increased, since the date of the use of shock wave therapy in the field of urology for lithotripsy and its effects have been better understood. Currently, ESWT is actively used in orthopedics and traumatology clinics in the treatment of many different musculoskeletal pathologies. In the literature, the applications mainly focus on bone, tendon, and soft tissue. The first applications on bone tissue started with nonunion and delayed healing case series,[2-5] followed by applications on osteochondrosis dissecans, osteonecrosis, bone marrow edema.[8,9] Applications on tendon tissue are often performed on plantar fasciitis.[10,11] Achilles tendinopathy,[4,12] calcifying tendinitis and lateral epicondylitis.[14,15] On the other hand, soft tissue applications focused on chronic wounds, scar tissues and hypertrophic wounds.
The high-amplitude sound waves (shock waves) used in ESWT is the result of a transient pressure change resulting from a sudden increase in ambient pressure in three-dimensional space. These shock waves have a peak pressure of about 1,000 times higher in terms of their physical properties than ultrasound waves. It is known that the effect of shock waves on the tissue occurs in four phases. In the physical phase, extracellular cavitation, ionized molecules, and membrane permeability increase due to the direct effect of shock waves. In the physicochemical phase, interaction occurs with spreadable radicals and biomolecules. In the chemical phase, intracellular reactions and molecular changes occur and, finally, the biological phase occurs.
Two types of focused (f) and radial (r) extracorporeal shock waves (ESW) are used in the clinic. In focused ESW (fESW), shock waves from a large shockwave source are directed to a single targeted point, whereas in radial ESW (rESW), shock waves from the source propagate as expanding waves in three-dimensional space and reach the targeted point and surrounding regions (Figure 1).
Wound healing refers to a complex process in which inflammatory reactions, proliferation and remodeling occur. In the proliferative phase of wound healing, collagen synthesis increases with rapid fibroblast proliferation in response to chemotactic factors synthesized during the inflammatory phase. In addition, capillaries formed by angiogenesis contribute to the formation of granulation tissue. In the remodeling phase, collagen synthesis is maintained by fibroblasts and wound healing is completed. Several studies have shown that ESWT increases the growth rate of fibroblast via messenger ribonucleic acid (mRNA) expression level and increases collagen type I and type III synthesis in fibroblasts in a dosedependent manner. These increase the interest in ESW application in the treatment of wound healing problems.[16,17,22-24]
There are theories related to the cellular explanation of how shock waves increase wound healing; however, there is no consensus in the literature. In a limited number of studies, it has been shown that ESW application may have a cytotoxic effect and it has been suggested that this is caused by both the mechanical cavitation effect and triggering the pro-inflammatory response and catabolic process in cells. As a result of this process, tissue healing mechanisms have been proposed to be activated.
In the present study, we hypothesized that ESW application had genotoxic effects on cells. We, therefore, aimed to evaluate wound healing effects of in vitro rESW application on mouse fibroblasts and whether the cytotoxic effect of ESW was due to a possible genotoxic effect. To the best of our knowledge, this is the first study in the literature to examine possible genotoxic effects of in vitro rESW application on mouse fibroblasts.
Patients and Methods
This study was approved by the Başkent University, Faculty of Medicine University, Institutional Review Board (No: 94603339-604.01.02/1985).
The L929 mouse fibroblasts (CCL-1, ATCC, Rockville, USA) were cultured in RPMI 1640 medium (Biochrome AG, Berlin, Germany) supplemented with heat inactivated 10% fetal bovine serum (FBS; Biochrom AG, Berlin, Germany), and antibiotic mix (10,000 U/mL penicillin and 10,000 μg/mL streptomycin, Biological Industries, Israel) in a 95% humidified incubator (Heraeus Deutschland GmbH & Co. KG, Hanau, Germany). Cells were subcultured every 24 h and cells at the 5 to 10 passage level were used in the study.
The shock-wave generator (Masterpuls® MP100; Storz Medical, Switzerland) used in orthopedics and traumatology clinic used for the in vitro experiments. Shock wave application was performed using a 15-mm diameter radial shock wave transmitter (Model No: R15, Storz Medical), which has a tissue penetration of ≥30 mm and has proven to have a therapeutic effect. The shock wave applications were performed as previously described with minor modifications (Figure 2). Briefly, cells were seeded in a 9 cm2 sterile Petri dishes. After cells were reached 95% confluency, they were stimulated with a frequency of 3 Hz and 100, 250, 500, 1,000, and 1,500 pulses of shock waves. Energy flux densities ranging from 0.01 to 0.23 mJ/mm2 (14.3 MPa) at a constant pressure level of 0.5 and 1 bar were applied. This experimental protocol was determined by examining the number and frequency of shock wave pulses used in previous studies to make a detailed evaluation in cell culture.[2,16,26-28] Additionally, separate cell cultures are used for each pulse shock and pressure level. Energy transfer from the radial (r)ESWT transmitter to the Petri dish was maximized by coating the surface of the Petri dishes with coupling agent. The rESWT application was performed at 24-h intervals, until the in vitro wound sites were closed (for two days). The cell cultures to be used in the study were, then, plated and an in vitro wound model was created, and the rESWT was not applied to the cell cultures in the control group. Evaluation of in vitro wound healing in the control group was performed blindly by a researcher familiar with this method, but not involved in the study to avoid bias.
In vitro scratch assay (wound healing)
The L929 cells were seeded in a Petri dish, and scratch wounds were made using a sterile 0.1 to 10 µL pipette tip in fibroblast cell culture and, then, the closure time and percentage of the scratch wounds were evaluated as previously described. Scratch wounds area was photographed using an inverted microscope (Olympus IX73, Japan) at 24-h intervals and analyzed by ImageJ version 1.53k14 (University of Wisconsin, Madison, WI, USA) software. For quantification, the area in the wound edges was measured at least of four areas for each application, and the mean values were calculated (d). The percentage of wound healing (WH) was calculated as follows:
WH%=[(doriginal wound-dhealing)/doriginal wound]X100
Under in vitro conditions, scratch wounds that do not have any rESW treatment close within 48 h (Figure 3). Therefore, we determined the follow-up period as 48 h in our study.
Determination of cell viability
Cytotoxic effects of rESWT application were determined using 3-[4.5-thiazol-2-yl]-2.5-diphenylte trazolium bromide (Sigma-Aldrich Inc., St Louis, MO, USA). Briefly, following the application in specified time and conditions, 5 μL of 5 mg/mL MTT were added to total of 1¥104 cells (final volume 0.59 mg/mL) and the cells were incubated at 37°C for 4 h. At the end of the incubation, 100 μL 10% of sodium dodecyl sulfate solution was added to cells and a final incubation step was carried out at 37°C for 16 h. Optical density of the chromogenic product was determined at 540 nm in a spectrophotometer (Epoch™; BioTek Instruments Inc., VT, USA) and viability of cells was calculated using spectrophotometer outcomes.
Assay for genotoxicity (Comet assay)
Genotoxic effects of rESWT application were determined by alkaline single-cell gel electrophoresis method (SCGE; comet assay) as previously described. Briefly, trypsinized cells were resuspended in phosphate-buffered saline (PBS) and mixed with 1% (w/v) low melting point agarose (LMPA; Sigma-Aldrich Corp., MO, USA). After this step, the cells were spread out on to the pre-coated slides with 0.5% (w/v) normal melting point agarose (NMPA; Sigma-Aldrich Corp., MO, USA). For the solidification of agarose slides placed with coverslips were put on ice packs. After the solidification of agarose coverslips were removed and third layer of LMPA was added on to the slides. After the incubation in lysis solution (10 mM Tris, 100 mM ethylenediaminetetraacetic acid (EDTA) disodium salt and 2.5 M sodium chloride; pH 10) for 2 h at 4oC (dark), slides were incubated in an electrophoresis buffer (1 mM EDTA disodium salt, 300 mM sodium hydroxide; pH >13) for 20 min in the dark in an opaque electrophoresis tank. Following the electrophoresis which was carried out at 300 mA for 30 min, slides were neutralized (0.4 M Tris; pH 7.5) and stained with ethidium bromide (2 μg/mL). One hundred nuclei were blindly scored using a fluorescence microscope (Nikon, Eclipse 600, Japan) and this process was repeated three times for each treatment. Thus, a total of 300 nuclei were scored. By the visual scoring, nuclei were categorized regarding to shape and comet tail. Undamaged, i.e., intact nuclei have globular shape were scored as 0, extremely damaged nuclei were scored as 4+ (Figure 4). Each counted nucleus was multiplied by its score, and total scores were expressed as arbitrary units (AU).
Statistical analysis was performed using the IBM SPSS for Windows version 25.0 software (IBM Corp., Armonk, NY, USA). Descriptive data were expressed in mean ± standard deviation (SD), median (min-max) or number and frequency. Normality assumption was tested using the Kolmogorov-Smirnov normality test. After evaluating whether the data were suitable for the parametric test, t-test was used for parametric data and Wilcoxon signed-rank test was used for non-parametric data. Analysis of variance was used in factorial order for comparisons of the means. If the prerequisites of parametric tests (analysis of variance in factorial order) were not met, the data were analyzed with the general linear model. A two-tailed p value of <0.05 was considered statistically significant.
Effects of rESW on wound healing (In vitro scratch assay)
When the control group and the 0.5 bar pressure group were compared, the wound healing rate at the 24 and 48 h decreased, regardless of the number of shots. However, when the control group and the 1 bar pressure group were compared, the wound healing rate decreased at 24 and 48 h, similarly to the 0.5 bar applied group, regardless of the number of shots (Figure 5). The p values obtained as a result of statistical comparison of both groups with the control group are given in Table I.
|Control vs.||0-24 h||0-24 h||0-48 h||0-48 h||24-48 h||24-48 h|
|SD: Standard deviation; * Paired t-test; ** Wilcoxon signed-rank test.|
Effects of rESW on cell viability
According to the general linear model analysis, when 100 shots were applied in the 0.5 and 1 bar pressure group, there was no significant difference in viability between the control group and the experimental groups (p=0.122). When ≥250 shots were exceeded, the viability decreased significantly after the 24 h compared to the control group, regardless of the pressure (Table II). The lowest viability values were reached in 1,500 shots at each pressure level (Figure 6).
|Control vs.||p||Mean difference|
|Cell viability (24 h to 48 h)||100 shots||0.122||0.049|
|* Statistical significance at p<0.05.|
Effects of rESW on genotoxic damage (Comet assay)
In vitro genotoxic damage was assessed at both 0.5 and 1 bar pressures, in both time intervals, regardless of the number of shots. Genotoxic damage was increased progressively from 24 to 48 h. The results are shown in Table III.
|24 h||48 h|
|0.5 bar||1 bar||0.5 bar||1 bar|
|SCGE: Single-cell gel electrophoresis; SEM: Standard error of the mean.|
Genotoxic damage observed in 24 h at 0.5 bar and 100 (p=1.000), 250 (p=0.558), 500 (p=0.135), and 750 (p=0.099) shots were similar to the control group, while significant genotoxic damage was observed in the 1,000 and 1,500 shots. On the other hand, higher genotoxic damage rate was detected at the end of 48 h in both groups compared to the control group (Table IV).
|24 h (p-values)||48 h (p-values)|
|Shots||Mean square||F||Significance||Mean square||F||Significance|
|0.5 Bar vs. 1 pressure||100||208.33||8.89||0.014*||705.33||21.07||0.001*|
|* Paired t-test; ** Wilcoxon t-test.|
When the pressure was increased to 1 bar, a significant genotoxic damage occurred even at 100 shots, unlike 0.5 bar pressure application in the 24-h evaluation. A significant genotoxic damage occurred in all groups below this pressure, regardless of the number of shots and the duration (Table IV).
In addition, the univariate analysis of variance revealed the genotoxic damage per shot count with 1.0 bar pressure which was significantly higher than the genotoxic damage per shot with 0.5 bar pressure (Table V).
|Control vs.||24 h||48 h|
|SE: Standard error.|
The positive effects of ESWT in many areas, particularly in the musculoskeletal system and chronic wounds, led to the investigation of the physical and biological effects of this method at the cellular and tissue level. Several studies in the literature have mainly evaluated the effects of fESW, and there are many questions to be answered about the molecular and cellular effects of rESW.[16,19,25,26,31]
In the current in vitro study, we showed rESW application reduced cell viability and delayed wound healing independently of the pressure level. The lowest viability values reached in the highest number of shots at each pressure level and time interval. In addition, in this study, for the first time in the literature, we demonstrated the genotoxic effect of shock wave application on fibroblasts under in vitro conditions using the comet assay. An increase in comet assay scores was accepted as an increase in genotoxic damage. In cell culture, a gold-standard protocol for rESW application has not been established; therefore, we determined a wide range of shock wave numbers to better demonstrate the rESW effects.
The increasing clinical use of ESWT in recent years has aroused interest in its effects on wound healing and wound care. In their study, Aschermann et al., after applying 0, 375, 750, and 1,500 pulses of rESW, waited 18 to 24 h for the detachment and re-attachment of the cells from the plate and, then, they formed the in vitro wound assay. The authors showed that fibroblast migration increased and, thus, in vitro wound healing increased in all groups after 48 h of follow-up. Contrary to their results, we showed in vitro wound healing (fibroblast migration) decreased in all groups, regardless of the number of shots. Although in our study, it was confirmed that fibroblasts did not separate from the base after each rESW application, the reason for this difference between the results may be that we first created the scratch assay and then performed rESW application. In addition, we believe that the reason for the decrease in fibroblast migration in our study is the decrease in viability and changes in the cytoskeleton due to the effect of cavitation. On the other hand, only fibroblasts are evaluated in the in vitro scratch assay. However, many cells such as neutrophils and macrophages play an active role in in vivo wound healing. Tepekoylu et al. showed that shock wave therapy increased macrophage recruitment to the wound area by increasing the pivotal macrophage recruitment factors such as macrophage migration inhibitory factor and macrophage inflammatory protein 1 beta. The effect of shock wave therapy on enhancing in vivo wound healing may be due to the contribution of cytokines secreted from increased macrophages to the wound healing process.
In the literature, there are studies examining the effects of rESW application on cell viability. Hochstrasser et al. examined the effect of rESW application in an in vitro study using human fetal foreskin fibroblasts (HFFF2). In their study, fibroblasts stimulated with a frequency of 1 Hz and 100, 200, 500, and 5,000 pulses shock waves were applied at a 2.5-bar pressure level. Cell viability was evaluated with the trypan blue exclusion assay. Viability decreased within the first 1 to 2 h after the application, regardless of the number of shock waves. In another study in which human dermal fibroblasts were used, 300, 1,000 and 2,000 pulses shock waves were applied and, 1 h after the application, fibroblast viability was evaluated by using MTT method. It was reported that viability decreased independently of the energy level and the greatest decrease was observed in the highest number of shock waves. Studies in the literature have also emphasized that with the increase in the number of shock waves applied, the viability decreases, and the main determinant of the viability is the shock wave number. In the current study, we showed that rESW application reduced cell viability compared to the control group independently of the pressure level when 250 or more shots were applied, and the lowest viability was achieved at the highest number of shots at both pressure levels. Therefore, it would be appropriate not to exceed 100 shots in rESW studies that are desired to be performed without changing cell viability. Our results seem to be compatible with previous studies.[16,19,25,26] The early cytotoxic effect seen immediately after rESW application suggests that rESW causes cell death by creating mechanical cell damage mediated by cavitation effect. The possible cause of cytotoxicity may be an increase in cell membrane permeability as a result of the direct effect of the shock wave in the first phase of ESW application, as well as acute disorganization of the cytoskeleton that cannot be repaired.
There are many studies in the literature investigating the effects of rESW application on different cell types. These studies usually evaluate cell viability, effects on cell proliferation, chemokine, and cytokine responses to shock wave application, activating and inhibiting cellular pathways, changes in gene expression, while there is no study on the genotoxic effect of shock wave on the cell in the literature.[34-36] In this study, we demonstrated the genotoxic effect of shock wave application on fibroblasts by the comet assay. According to our results, regardless of the number of shock waves applied, genotoxic effects were observed at the end of 48 h in both pressure groups. In the in vitro study of Ashermann et al., fibroblasts increased gene expression and proteins that regulate the cell cycle in response to the shock wave, thereby attempting to achieve genome stability. These findings are also consistent with our study. Genotoxic damage can be caused by direct physical effects, permeability changes, ionizing molecules and resulting soluble radicals created by ESW application on the cell. In addition, high-energy shock wave application may cause apoptosis or necrosis through genotoxic damage. According to the results obtained from this study, the severity of the genotoxic damage was directly affected by the pressure increase and 1,000 shots at 0.5 bar pressure were considered as the threshold value for genotoxic damage in in vitro conditions. Since the genotoxic effect of the application up to 1,000 shots at 0.5 bar pressure occurred significantly at the 48 h, it was thought that this application might stimulate apoptosis in the cells. On the other hand, genotoxic damage occurring in the first 24 h in all groups may be associated with necrosis. Therefore, we recommend staying below 1,000 shots for therapeutic effect studies and using shots above 1,000 at 0.5 bar or, regardless of the shot number, 1 bar pressure should be used in experimental studies to induce genotoxic damage. Mechanisms of genotoxic damage caused by ESW application should be clarified in future studies.
More intriguingly, in an experimental study of rats with spinal cord damage, low-energy ESW application increased angiogenesis by increasing vascular endothelial growth factor expression in nerve cells, thus improving locomotor and sensory functions. Finally, in an in vivo study, Haberal et al. reported that shock wave therapy applied in rats with lumbar laminectomy reduced epidural fibrosis. The reason for the decrease in epidural fibrosis in this study may be the fibroblast death due to the genotoxic damage observed in the current study, and the possible effect of inflammation triggered by this cytotoxic effect on wound healing.
Nonetheless, this study has some limitations. Our research is based on in vitro experimentation and cannot be linked to in vivo conditions. In vivo wound healing is a complex process and not only through fibroblasts, and it depends on tissue architecture and composition of extracellular matrix. With chemokines and cytokines secreted from endothelial cells, cell-cell interactions and the barrier effect created by living tissues and changes in tissue integrity are both effective on in vivo results. In addition, different experimental setups can be used in in vitro rESW applications. Water bath setup, which is the method frequently used in the literature, was not used in this study, that may have affected the experimental results. Finally, comparing the results obtained from the in vivo study to be performed simultaneously with the in vitro study could provide a better examination of the mechanism of action.
In conclusion, the present study demonstrated the effect of rESW application on fibroblast viability, wound healing and fibroblast genotoxicity using MTT assay, in vitro scratch assay, and comet assay. According to these results, wound healing was delayed and cell viability decreased at all pressure levels, all shot numbers, and all time intervals in fibroblast cultures applied rESW in the in vitro setting. In addition, the severity of genotoxic damage increased proportionally with the increased pressure level. We believe that this study is valuable, as it is the first to reveal the genotoxic effects of rESW application in vitro. By using different energy and impulse regimes and in vivo studies, more useful data can be obtained and the effects of rESW application can be clearly demonstrated.
The authors declared no conflicts of interest with respect to the authorship and/or publication of this article.
This study was approved by Baskent University Institutional Review Board (Project no: DA18/32) and supported by Başkent University Research Fund.
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