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1.IntroductionThe tympanic membrane (TM) separates the outer ear canal from the middle ear.1 Its function is to collect the sound that has been transmitted through the ear canal, amplify it and transmit it further through the ossicular chain to the inner ear.2,3 The TM layer facing the outer ear canal is represented by the slightly keratinized epithelium (epidermal layer) and the subepidermal layer of loose connective tissue. The median layer, called lamina propria, is the collagen rich structure of the TM consisting of a radiar (external) and circular (internal) collagen layer. The predominant type of collagen within the pars tensa is collagen type II.4 The TM layer facing the tympanic cavity consists of the monolayered epithelium (mucosal layer), which covers the tympanic cavity as well [Fig. 1(c)].5–8 As a common deficiency after chronic affections involving the eardrum and TM perforations, the TM often heals with atrophic scars. These atrophic parts of the TM are thinner than the nonaffected TM and have a deficiency in fibroblasts and the collagen layer.9,10 Depending on the dimensions of the atrophic area of the TM and the ventilation of the tympanic cavity, different conditions appear: (1) localized atrophic scar, (2) TM retraction pocket, and (3) atelectasis of the tympanic cavity.11–15 To prevent the development of cholesteatomas, the further major and life endangering complication of these pathologies, and correct conductive hearing loss, the surgical intervention (tympanoplasty) is currently the state-of-the-art therapy complemented with measures that improve the Eustachian tube function. Laser irradiation of different types of tissues—such as the basilar membrane of the cochlea,16 the cornea,17 the femoropatellar joint capsule,18,19 the medial collateral ligament,20 the periodontal ligament,21 and the skin22—is known to induce conformational changes in the structural collagen. Although in the first period after irradiation, a decrease in the tissue stiffness can be observed,18,20 a consequent increase in the tissue stiffness follows after days to years due to collagen remodeling.20,23–25 The question arises therefore if this method could be used for collagen remodeling within the TM as well. Kurkowa and Goode13 first proposed the use of lasers to tighten atrophic TM13 demonstrating the contraction of these pockets in explanted human temporal bones. Later, Ostrowski and Bojrab,14 Brawner et al.,15 and Ryen and Kaylie12 performed the first clinical studies. However, this idea did not make it to the routine therapeutic strategy due to the need of further studies.12 We therefore proposed to assess the laser treatment to induce collagen remodeling within the TM in an animal model and use the advantage of comparing the effects of different applied laser intensities from histological and electrophysiological point of view before entering clinical studies. Additionally, we applied pigments to reduce the light energy needed and exactly define the borders of the TM areas to be remodeled, while leaving the rest unaffected. This could be the prophylactic intervention in an early stage of the disease, that would stop the process and avoid a later surgical procedure, having the advantage of very confined tissue remodeling to the affected area, using lasers. 2.Material and MethodsWenzel et al.26 demonstrated that 2 weeks after laser irradiation of the basilar membrane within the cochlea, collagen remodeling, and new collagen deposition could be observed. Based on these studies, we designed our herein presented method for laser irradiation of the TM and its electrophysiological and histological results in an animal model. 2.1.Animals85 female CD1 albino mice, weighing 20 to 30 g at the age of 5 to 8 weeks were used for this study. Out of these, the temporal bones of 74 animals were processed for the analyses with transmitted light and polarized light microscopy, and 11 animals for transmission electron microscopy (TEM). Auditory brainstem responses (ABRs) were recorded to monitor hearing. 2.2.Surgical TechniqueThe “Saarländische Landesamt für Verbraucherschutz” approved the study protocol in accordance with the “Deutschen Tierschutzgesetz und der Richtlinie des Rates der europäischen Gemeinschaft zum Schutz der für experimentelle Zwecke verwendeten Tiere.” The mice were anesthetized with an intraperitoneal injection ( BW) of 2.125 ml 0.9% isotone solution of sodium chloride, 0.25 ml ketamine, and 0.125 ml rompun. During the experiment, the body temperature was maintained at 38°C using an electric heating pad. After trimming the hair around the ear, we performed a 2-mm long incision beginning at the incisura intertragica and extending it along the cartilaginous outer ear canal exposing the TM on both sides. After recording ABR, the external ear was anchored with sutures to expose the entire TM. To enhance the laser energy absorption and achieve optical selectivity for the proposed defined part of the TM, we stained the target area of the posterior (post) superior quadrant (diameter ca. ) with the pigment Fuchsin (0.5% solution with alcohol, pharmacy, Saarland University), a water-soluble solution that has its maximal optical absorption at 455 to 600 nm.27,28 We stained the contralateral ear as well as a control. The anterior (ant.) part of the TM was, on both sides, not touched. After staining, we irradiated the marked area on the left TM (Fig. 1). The ABR thresholds were then recorded again and the incisions on both ears sutured. Until fully awake, the mouse was monitored and put under an infrared lamp to protect it from hypothermia. After 14, 28, or 56 days, according to the respective test group, the mice were anesthetized again, the incisions on both ears reopened and final ABR thresholds were measured. The animals were then sacrificed through cervical dislocation under deep anesthesia. The petrous part of the temporal bone was extracted ex vivo and the tympanic cavity opened and perfused with fixative. 2.3.Laser IrradiationWe used a 532-nm pulsed neodynium-doped yttrium orthovanadate () (Xiton Photonics GmbH, Kaiserslautern) as the laser source. The pulsed laser light was applied through a laser fiber with a diameter of that we directed to the stained area of the TM with a micromanipulator. We estimated the distance as close as visible possible to the stained area, without touching the TM, giving an irradiation diameter of on the TM. The final position adjustment has been performed using a continuous waved pilot laser, with a power of 0.1 mW, for a maximum of 30 s (Fig. 1). We then irradiated the stained area of the TM for 30 s with a power of either 10 mW (0.3 J), 25 mW (0.75 J), or 50 mW (1.5 J) at a laser repetition rate of 2 kHz (Table 1). Table 1Summary of the analyzed animals with focus onto the irradiation duration, intensity, and total dose of laser energy applied as well as the day of sacrifice.
2.4.Electrophysiological Monitoring: ABRWe used a digital signal processing system that generated sine wave stimuli (Agilent 33500 B Series Trueform Waveform Generator, Keysight Technologies GmbH, Germany) and delivered them through a free-field speaker (Beyerdynamic GmbH & Co. KG) placed in front of the mouse at 5 cm distance to each ear. With this system, we recorded click- and frequency-specific ABRs using four needle electrodes: one on each mastoid, one at the vertex (reference), and one at the base of the tail (ground). The recorded signals were then amplified through the biosignal amplifier (g.USBamp, g.tec medical engineering GmbH, Austria), digitized at 19.2 kHz and digitally filtered to obtain the frequencies in the 300 to 2500 Hz range. The stimulus intensities ranged from 0 to 80 dB SPL increased in 10 dB steps at 2, 4, 8, 12, 16, 20, 32, 48, and 80 kHz. We estimated the hearing thresholds for each recording visually, offline and defined it as the lowest intensity, where the Jewett complex was identifiable. Additionally, within the click ABR data, we measured the amplitude and latency of the wave I peak to peak.29 2.5.Transmitted Light MicroscopyWe explanted the temporal bones, opened the tympanic cavity, and fixated the samples with a 4% formaldehyde for 2 days. We performed the decalcification in 20% EDTA with 100% citric acid (pH 7.2) for 4 days, dehydrated them in ascending ethanol series of 70% and 100% (360 min), placed them in 100% Xylol (180 min), and finally embedded them in paraffin. Afterward, we cut the blocks in sections and stained with hematoxylin–eosin to get a first impression of the anatomy. We then used the picrosirius red staining (Sigma-Aldrich Chemie GmbH, München) (MORPHISTO® Evolutionsforschung und Anwendung GmbH, Frankfurt) to analyze the morphological changes within the TM. For transmission microscopy, we used three to four slides of each ear. The interval between each utilized slide-series was . We then measured the thickness of the posterior part of the TM from the left (irradiated) and the right (nonirradiated) ear as a control (Fig. 1 dashed squares). 2.6.Polarized Light MicroscopyWe used picrosirius red and added hemotoxylin to enhance the natural birefringence of collagen and visualize regions with just a minimal quantity of collagen.30,31 Picrosirius red is an elongated, birefringent molecule, which binds parallel to collagen molecules being used to identify and characterize collagen structures within biological tissues.17,30,32–34 The sections were then visualized and imaged under polarized light microscopy. To ensure that the settings of the microscope were always the same, we started with a control ear and rotated the polarizers until the birefringence of the tissue was maximized. Furthermore, the remaining microscope settings were optimized. Once this was done, the polarizers were locked and the light exposure, the aperture size, the position were also held constant for all the other slides and images captured. We used ImageJ (National Institutes of Health) to quantify the highest intensity of birefringence analyzing areas of 3000 to 4000 pixels within the irradiated and the corresponding control TM. 2.7.Transmission Electron MicroscopyFor a more detailed analysis of the structural changes within the TM, 4 weeks after irradiation, we used TEM. The explanted petrous bones were fixed for 1 day in 1% glutaraldehyd in 0.1 M cacodylate buffer containing 1% paraformaldehyde and at a pH 7.2 to 7.4 and afterward decalcified in 20% EDTA for 6 days, washed with 0.1 M cacodylat buffer, and fixed with 0.2% osmium tetroxide. As a next step, the samples were washed in distillated and gradually dehydrated from 80% to 100% ethanol and three times stained with acetone, two times with epon (3:1, 1:1, 1:3), and subsequently embedded in pure epon followed by polymerization for 2 days at 60°C. After cutting them in about 70-nm thin sections with an ultramicrotome (LEICA EM UC7, © 2015 Leica Biosystems, Nussloch), they were positioned on a copper grid, contrasted with 2% uranyl acetate, postcontrasted with lead citrate, and analyzed with a transmission electron microscope (FEI TECNAI 12, The Netherlands). 2.8.Statistical MethodsWe used SPSS and performed all tests at an alpha level of 0.05. The hearing thresholds for the click stimulation as well as for the frequency-specific stimulation, as described in Sec. 2.2, were analyzed with a nonparametric test (Friedman). Additionally, we conducted a repeated measure analysis of variance (rmANOVA) for the factor “power” and an rmANOVA for the factor “weeks” using Huynh–Feldt correction for the degrees of freedom. For the analysis of wave I of the ABR recordings, the TM thickness, and the TM polarization, we conducted a one factorial ANOVA, followed by a Bonferroni posthoc test to compare the individual groups. We also performed a Levene test of variance homogeneity. If this turned to be significant, we performed a more robust test, the Welch ANOVA, followed by a Games-Howell procedure as posthoc test. Additionally, in the cases when the data were not distributed normally, we performed a nonparametric test, the Friedman test, followed by a Bonferroni posthoc test. 3.Results3.1.Transmission Light MicroscopyThe thickness of the TM increased with increasing intensity of irradiation (Fig. 2). This demonstrated to be valid and statistically significant for the animals exposed to 25 mW for 30 s (0.75 J) and 50 mW for 30 s (1.5 J) independent of the time postexposure. The animals exposed to 10 mW for 30 s (0.3 J) did not have any increase in TM thickness in comparison to the contralateral nonexposed ear. To quantify these changes, we subtracted from the thickness of the stained and irradiated area of the (left) TM, the thickness of the same area of the stained nonirradiated (right) ear in each animal, and plotted the averaged results of these differences (Fig. 3). The maximal increase in TM thickness could be observed for the group of mice irradiated with 50 mW for 30 s (1.5 J) and sacrificed after 2 weeks. Even though the trend was toward an increase in thickness with the increase in optical power applied, this change was, however, statistically significant just between 10 mW for 30 s (0.3 J) and 25 mW for 30 s (0.75 J) or 10 mW for 30 s (0.3 J) and 50 mW for 30 s (1.5 J) but not significant between 25 mW for 30 s (0.75 J) and 50 mW for 30 s (1.5 J). This effect could be observed at all time points of sacrifice 2, 4, or 8 weeks. The mice who were sacrificed after 2 weeks demonstrated a significant increase in the TM-thickness between the groups irradiated with 10 mW for 30 s (0.3 J) compared to the once irradiated with 25 mW for 30 s (0.75 J) () and 50 mW for 30 s (1.5 J) (), but no significant change between the mice irradiated with a power of 25 mW for 30 s (0.75 J) to the group irradiated with a power of 50 mW for 30 s (1.5 J) (). The mice sacrificed after 4 weeks demonstrated a significant increase of the TM thickness between the group irradiated with 10 mW for 30 s (0.3 J) to the groups irradiated with 25 mW for 30 s (0.75 J) () and 50 mW for 30 s (1.5 J) (). Again, no significant TM thickness increase could be observed between the mice exposed to 25 mW for 30 s (0.75 J) and the ones exposed to 50 mW for 30 s (1.5 J) (). Similar to the mice sacrificed after 4 weeks, the mice sacrificed after 8 weeks demonstrated a significant change in TM thickness between the 10 mW for 30 s (0.3 J) irradiated mice to the 25 mW for 30 s (0.75 J) (), and 50 mW for 30 s (1.5 J) () animals, however, no significant change in the TM thickness of mice exposed to 25 mW for 30 s (0.75 J) compared the ones exposed to 50 mW for 30 s (1.5 J) () (Fig. 3). Additionally, we compared the sections cranial (1) and caudal (3) to the stained and irradiated area (2) of the TM (Fig. 1). The analysis demonstrated that a tissue proliferation was induced just in the area of the stained and irradiated part of the TM (). The parts above and underneath this area were not significant different to their stained and nonirradiated controls (contralateral ear) (). 3.2.Polarized Light MicroscopyWe analyzed the TMs birefringence as an estimation of the build/remodeled collagen using polarized microscopy, as described in Sec. 2.6 (Fig. 4), and compared the birefringence of the stained and irradiated area of the left TM with the same area of the control-right TM (stained and not irradiated). The mice irradiated with 25 mW for 30 s (0.75 J) or 50 mW for 30 s (1.5 J) demonstrated after 4 and 8 weeks an increase of the TM birefringence. The statistical analysis demonstrated that this increase was statistical significant 4 weeks postirradiation: () for 25 mW for 30 s (0.75 J) and () for 50 mW for 30 s (1.5 J), however, not significant between the animals irradiated with 25 mW for 30 s (0.75 J) to the 50 mW for 30 s (1.5 J) (). The incubation time of 2 weeks did not induce a statistical significant change in the TM-polarization either () (Fig. 5). Within the mice groups, which were sacrificed after 8 weeks, a significant increase in birefringence could be demonstrated between the mice group irradiated with 10 mW for 30 s (0.3 J) and the ones irradiated with 25 mW for 30 s (0.75 J) () as well, however, no significant change between the 25 mW for 30 s (0.75 J) irradiation and the ones irradiated with 50 mW for 30 s (1.5 J) (). Interestingly, despite the clear trend toward increase in birefringence with increasing energy, the statistical analysis revealed no significant increase in birefringence between the mice irradiated with 10 mW for 30 s (0.3 J) and 50 mW for 30 s (1.5 J) (). After exposing the stained TMs to 10 mW for 30 s (0.3 J), the increase of birefringence was not statistically significant either (Fig. 5). Over time the increase in birefringence was significant within the first 4 weeks for the animals irradiated with 25 mW for 30 s (0.75 J) () and 50 mW for 30 s (1.5 J) () followed by a stagnation within the next 4 weeks (nonsignificant increase in birefringence in the mice irradiated with a power of 25 mW for 30 s (0.75 J) () and 50 mW for 30 s (1.5 J) ()). The animals irradiated with 10 mW for 30 s (0.3 J) had no significant increase in birefringence (). As expected, a significant increase in birefringence was observed in the main stained and irradiated Sec. 2 of the TM ( when comparing the irradiated to the nonirradiated control and for the difference between Secs. 1 and 2 and for the comparison of Secs. 2 and 3). The birefringence within the area of the outer Secs. 1 and 3 did not differ significantly (). 3.3.Transmission Electron MicroscopyThe nonirradiated TMs [Figs. 6(b), 6(d), and 6(f)] revealed the typical three layered structure.7,8 Within the TM irradiated with 10 mW for 30 s (0.3 J) [Fig. 6(a)], we observed a slight change in the radial organized collagen layer, which seemed to be arranged more loosely and was slightly interspersed with circular collagen fibers. Within the TM irradiated with 25 mW for 30 s (0.75 J) [Fig. 6(c)], the new circular structured collagen fibers appeared to be at least doubled compared to the contralateral, nonirradiated TMs. In addition, the ratio between the different collagen layers appeared modified with a larger increase in the circular structured collagen. Within the TM irradiated with 50 mW for 30 s (1.5 J) [Fig. 6(e)], the reorganized collagen layers demonstrated a further increase in thickness and the delimitation between the different organized collagen layers was loose. 3.4.Measurement of ABRThe click-ABR of each mouse demonstrated no significant threshold shift directly after irradiation. With our recording setup, no significant difference between the irradiated and the contralateral nonirradiated ear () could be recorded. The final click-ABR recordings demonstrated a threshold shift of 10 to 40 dB in 56 of 75 mice that was as well observed for both ears (the irradiated and the nonirradiated ears). The frequency-specific ABRs demonstrated similar results as the click-ABRs (Table 2). Twenty-five mice had in 1 to 2 frequencies a threshold shift at the second and third measurement compared to the first, both ears were affected. Nine mice were deaf from the start. The amplitude and latency of wave I did not present a major difference between the irradiated and the contralateral, not irradiated ear (). Table 2Frequency-specific ABR: significance analysis for the individual frequencies.
4.DiscussionWe herein present a preclinical study for a laser based collagen remodeling of the TM. To our knowledge, this is the first study analyzing the histological details of this process at the TM level. We demonstrate in an animal model, that depending on the intensity of the applied laser irradiation (10 to 50 mW for 30 s to 1.5 J) and the time of sacrifice (incubation time after irradiation), an unspecific increase in the tissue volume was induced in the TM (Figs. 2–6). The polarized light (Fig. 4) and the TEM (Fig. 6) revealed that this tissue volume change can be attributed to a laser induced collagen remodeling and collagen deposition, as described in other anatomical structures, such as the cornea,17 the femoropatellar joint capsule,18,19 the medial collateral ligament,20 the periodontal ligament,21,22 the skin,22 and the basilar membrane of the cochlea.26 To be noted that the mice irradiated with 25 mW for 30 s (0.75 J) and 50 mW for 30 s (1.5 J) demonstrated after 2 weeks a slight decrease of the TM-birefringence most probably through the initial disorganization of the collagen fibers in these cases. Additionally, no significant change could be observed between the animals irradiated with 25 mW for 30 s (0.75 J) to the 50 mW for 30 s (1.5 J) (), demonstrating no need to increase the laser energy up to high levels in order to induce collagen remodeling. Furthermore, we noticed that a specific amount of laser-energy is needed to induce the tissue-change we wanted. Too much energy, e.g., 50 mW for 30 s (1.5 J) induced strong inflammation observed after 2 weeks. Too low intensities (in our study, 10 mW for ) did not have any significant effect on tissue remodeling in the herein presented study [Figs. 2(a), 3, 4(a), and 5] even though, the TEM image in Fig. 6(a) demonstrated slight disorganization of the collagen layers. Additionally, a trend toward increase in birefringence at 8 weeks for the 10 mW for 30 s (0.3 J) irradiated ears could be observed that appeared however to be statistically not significant (Fig. 5). The TEM confirmed that 4 weeks after irradiation of the TM with 10 to 50 mW for 30 s (0.3 to 1.5 J), the histological structure of the collagen layer of the TM was reorganized and an unspecific collagen increase could be observed. Within future studies, more intensities, especially between 10 and 25 mW for 30 s (0.3 to 1.5 J), that would allow a finer quantification of the needed laser parameters and of the optimal pigment in order to achieve the desired collagen deposition, while minimizing the risk of a local inflammation, are needed. The other variable that we analyzed was the time after irradiation: 2, 4, and 8 weeks. As in previous research described, collagen remodeling is a process that takes from weeks up to several months.23–25 Shortly after the laser irradiation and especially using high intensity, an inflammation occurred.35 In our study, the collagen remodeling was significant as well starting with 4 weeks followed by stagnation within the following 4 weeks (Fig. 5). We also noticed that the pigment (Fuchsin used in this set of experiments) was essential to improve the laser absorption within the transparent structure of the TM in our animal model as well as inducing the irradiation effects in a defined area, where the surgeon would apply the pigment not changing the original structure of the rest. Additionally, this technique enabled us to keep the amount of applied light energy at low levels compared to previous studies from Kurkowa and Goode,13 who first proposed to use lasers to tighten atrophic TM in human temporal bones (laser energy settings ranging from 6.5 to (2 to 6 W). Ostrowski and Bojrab14 used a laser with laser power settings ranged from 0.1 to 1.0 W to induce contraction of TM retraction pockets in patients. Brawner et al.15 used a pulse diode potassium-titanyl-phosphate (KTP) laser (532 nm) with a diffuse beam and low power (800 to 1200 mW) mentioning the use of pigments in some of their patients, and Ryen and Kaylie12 used a laser at a power of 2 W to treat TM atelectasis. Even though at the beginning of the study, this was not the case, the pigment Fuchsin has been meanwhile demonstrated a carcinogenic effect.36 For this reason, the upcoming research will further define the optimal pigment-laser combination for assuring the biocompatibility of this technique. Shortly after irradiation, there was no increase in ABR thresholds. This finding was not dependent on the intensity of light applied confirming the decreased chance of toxicity with our used energy levels. Further experiments are however needed to clearly define the long-term effects for the hearing system including the testing of each ear independently. 5.ConclusionWe were able to induce a collagen remodeling through laser irradiation and histologically prove an increase in collagen in defined areas of the TM. Using a pigment that increased the absorption of photons we reduced the amount of needed light energy and left the structure of the rest of the TM unaffected. This method would allow keeping the natural undamaged structure of the TM while acting in a therapeutic way just onto the pathological changed areas of the TM. The best increase in TM thickness after laser irradiation of the stained TM could be observed and quantified within the first 4 weeks with no further statistically significant changes afterward in our dataset. Additionally, the intensity of irradiation seemed to be important, just up to 25 mW for 30 s (0.75 J), with no need of further increase in the applied energy. This is due to no further significant TM thickness changes, however, the risk of toxicity. To our knowledge, this is the first study reporting histological analyses of laser-induced changes within the TM. Additionally, the electrophysiological measurements that demonstrated no irradiation-dependent threshold shift sustain the noninvasive therapeutic character of this method. Further studies are on the way to analyze the local temperature increase that induces the collagen remodeling, the long-term effects of this therapy, as well as the exact stiffness of the eardrum after irradiation. Based on these studies, the optimal pigment/laser-parameters to be used could be optimized. Additionally, the study of these effects on an animal model of deficient TM would further complete the information for the clinicians. DisclosuresThe authors have no relevant financial interests in this article and no potential conflicts of interests to disclose. 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