- About this Journal
- Abstracting and Indexing
- Aims and Scope
- Article Processing Charges
- Articles in Press
- Author Guidelines
- Bibliographic Information
- Citations to this Journal
- Contact Information
- Editorial Board
- Editorial Workflow
- Free eTOC Alerts
- Publication Ethics
- Reviewers Acknowledgment
- Submit a Manuscript
- Subscription Information
- Table of Contents
Journal of Spectroscopy
Volume 2013 (2013), Article ID 903450, 6 pages
Raman Spectroscopic Analysis of H2O2-Stimulated Three-Dimensional Human Skin Models Containing Asian, Black, and Caucasian Melanocytes
1Cellular Informatics Laboratory, Advanced Science Institute, RIKEN, Wako 351-0198, Japan
2Department of Chemistry, School of Science and Technology, Kwansei-Gakuin University, Sanda 669-1337, Japan
3Kobe Technical Center, Procter and Gamble Japan, Kobe 658-0032, Japan
4Procter & Gamble International Operations S.A., Singapore Branch, Immunos No. 02-12, 8A, Biomedical Grove, Singapore
Received 11 September 2012; Accepted 17 November 2012
Academic Editor: Kong-Thon Tsen
Copyright © 2013 Shin-ichi Morita et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
Reactive oxygen species generated in dermal cells of human skin is related to skin disorders or diseases. In this study, Raman analysis effectively clarified the identities of three types of human skin models after the models were stimulated with hydrogen peroxide. With the Caucasian skin model, the major Raman bands underwent large intensity changes within 4-5 days of stimulation. With the Black skin model, the Raman bands remained almost unchanged. The changes in the Asian skin model were unique compared to those in the above two. Eumelanin and pheomelanin are probably the main compounds that differentiate dermal cells in terms of their sensitivity to hydrogen peroxide.
Human skin is sensitive to sunlight, especially to ultraviolet (UV) light, which generates reactive oxygen species (ROS) in dermal cells. This phenomenon is related to disorders or diseases such as stains, freckles, and cancers of the skin. Many researchers have sought to understand these disorders at the molecular level and are also interested in classifying them [1–3]. In clinical medicine, Raman spectroscopy attracts researchers as a microscopic, nondestructive, and nonlabeling research tool. Raman spectroscopy provides information about the compositions, structures, and interactions of molecules , and it has been used as a powerful analytical method in chemistry for 80 years. Its application to clinical medicine has been somewhat slower, beginning during the 1970s [5–7], when the development of a Raman microscope allowed effective spectral measurements of biological tissues [8–11]. Today, we can measure the Raman spectrum of a live cell (ca. 20 μm in width) with high spectral quality, distinguishing an area of 1 μm2 in the horizontal plane (ca. 30 s for the spectrum) [12, 13]. Moreover, the use of a flexible fiber is one of the most promising approaches for making noninvasive Raman measurements of living tissues, and several research groups have developed fiber optics suitable for Raman measurements [14–19].
In this study, three-dimensional (3D) human skin models were stimulated with hydrogen peroxide (H2O2) to provide time-dependent Raman spectra. As mentioned above, UV-visible light generates ROS in dermal cells. H2O2, one of typical ROS, was therefore used as a substitute for UV light to stimulate the skin models. The 3D human skin models consisted of keratinocytes, melanocytes, and a collagen-layered membrane, as shown in Figure 1(a), which are frequently used for skin irritation tests in dermatology. Three kinds of skin models, containing Caucasian, Asian, and Black type melanocytes, were used to simulate individual differences. Caucasian-type keratinocytes were used throughout the models.
The aims of this study were (i) to confirm whether the Raman technique is capable of detecting early chemical responses or the phenylalanine ring, CH2 bending, and amide I vibrations within a few days of H2O2 stimulation, in the skin models (because pigmentation is recognizable macroscopically only at around two weeks after stimulation) and (ii) to determine whether the Raman approach can clarify/distinguish the identities of these skin models. Our Raman approach successfully clarified the skin properties within 4-5 days after the H2O2 stimulation. Not only Raman measurements, we observed also the hematoxylin and eosin (HE)-stained visible images of skin models before and after the H2O2 stimulation and the absorbance values using the 405 nm visible light, to give a reasonable discussion. The results obtained in this paper are of importance since they will provide a bright future for a Raman method, mainly utilizing Raman bands of proteins, to enable the nonlabeling, noninvasive, and early diagnosis of human skin disorders.
Three kinds of 3D human skin models (MEL300 series) and growth medium (EPI-100 containing KGF113) were purchased from the Bio-Medical Department of Kurabo Industries Ltd. from MatTek Corp. Hydrogen peroxide (Wako Pure Chemical Industries, Inc.) was used to stimulate the skin models. A CO2 incubator was used to maintain the skin models at 37°C under a 5% CO2 atmosphere. Five pieces of the Asian skin model were subjected to H2O2 stimulation in which 10 μL of 2 mM H2O2 was added to the 5 mL of medium containing each piece of the Asian skin model. Another piece was used as the control, with no H2O2 stimulation. This procedure was repeated for both the Black and Caucasian skin models. Stimulation was applied once for each piece of a skin model.
A CCD-equipped Raman spectrometer (RS in Figure 1(b)) was used with a microscope attachment. Laser light tuned to 785 nm (L785) was reflected with an edge filter (EF). The laser power was averaged to 130 mW. The light was focused onto the target material with an objective lens (L1: 20×, NA 0.4). The scattered light of the target material reached the RS through L1, EF, a notch filter (NF), an imaging lens (L2), and a slit (S: 100 μm in width). For sufficient filtration of the light, the NF filter was placed perpendicular to the path. To establish the time course of the stimulation, as shown in Figure 1(c), the skin model samples were taken out of the incubator piece by piece to make the Raman measurements. We obtained Raman spectra at seven random locations, focusing on the surface of each skin sample avoiding apparent pigmentation spots. The focal point was chosen so that the Raman signal was maximum. The time for the measurement of a spectrum was 600 s (exposure 10 s, with 60 scans).
The Raman spectrum, which we called in this paper the “pure" spectrum, was calculated as , where , , and are the spectra obtained experimentally with the following procedures. (i) The spectrumwas obtained by irradiating the target material on an aluminum foil support with 785 nm light. (ii) The reference spectrum was measured by irradiating the aluminum foil with 785 nm light with no target material (the aluminum foil was placed above the focal point of the light). (iii) Another reference spectrum, , was obtained without laser irradiation by placing a white light source at the focal point. A tungsten lump was used as the white light source, and a pin hole was used so that the white light passing through it became a spot (0.9 mm in diameter). The attachment of a variable resistor connected to a battery allowed the light intensity of the light source to be adjusted.
The baselines of the pure Raman spectra were then corrected. The baseline-corrected Raman spectrum was calculated as , in which is a fitted polynomial curve constructed with the following procedures. (i) For a spectrum truncated between the minimum Raman shift position and the maximum position , the degree of the function was selected to fit the baseline using a polynomial function (this time ). (ii) Using the least squares method, the polynomial function was first fitted to the Raman spectrum . (iii) The Raman spectrum was divided into upper and lower parts, relative to the fitted baseline . (iv) The number of data points on the upper side of was designated , and the number on the lower side of was designated . If , the upper part of was removed from the whole of , and the Raman spectrum was replaced with the lower part of the spectrum. Then, procedure (ii) was repeated. When , the baseline was considered the best fit and optimal.
3. Results and Discussion
As explained in Section 1, human skin is sensitive to sunlight, especially to UV light, which generates ROS in dermal cells. In this research, one of ROS, hydrogen peroxide, was used as a substitute for UV light. Here, we confirmed that the pigmentation of the Black type skin model was reproduced by the stimulation of H2O2. Figure 2(a) shows the skin models containing Black type melanocytes without and with the stimulation of the H2O2 (10 μL of 10 mM H2O2 was added to the 5 mL of medium containing a single piece of the Black type skin model. The black type was here chosen to exemplify the pigmentation of the skin models since the existence of melanin was the most readily recognizable). The image of the skin model at a week after the stimulation gave several clear spots (almost Black in color) of melanin above the supporting layer (collagen) while that without the stimulation (the control) provided less spots of melanin. Also, we checked that the absorbance value at 405 nm of the skin model after the H2O2 stimulation was clearly increased compared to that of the control (Figure 2(b)).
Figure 3(a) shows all the pure Raman spectra produced in the present study. The offset values of the spectra differed greatly. When the background value of a spectrum was low, the corresponding baseline was close to a straight line. If a baseline shifted upward, it was varied to a more concave-down structure, and accompanying this change, the Raman peaks became more planar. In Figure 3(b), the spectra of each model were averaged over the time course. The offset values, wavenumber averaged, were ~0.24, ~0.16, and ~0.11 for the Black, Asian, and Caucasian models, respectively. These values are probably influenced by the eumelanin bio-polymers of human skin, which gives two broad peaks of Raman bands at 1580 and 1380 cm−1 whose full widths of half heights are around 100 cm−1 and whose positions are not influenced by the wavelengths of excitation lights (457.9, 514.5, 632.8, and 785 nm) .
Figure 4(a) shows the baseline-corrected spectra. The major bands at 1007 cm−1, 1455 cm−1, and 1662 cm−1 are assigned to the ring breath mode of phenylalanine, the CH2 bending mode, and the amide I mode of proteins, respectively [13, 21]. Figure 4(b) shows the time-dependent intensity profiles for these specific bands. For the Caucasian model, almost all the Raman bands underwent large intensity changes within 4-5 days of stimulation, and the bands became stable thereafter. For the Black model, the Raman bands remained almost unchanged throughout the observation period. For the Asian model, the spectral changes were intermediate compared with those of the Caucasian and Black models. The Raman responses of the Caucasian and Asian models that occurred within 4-5 days of H2O2 stimulation (Figure 4(b)) are both interesting and important because the phenomenon is probably relevant to the early-stage-sensing and diagnosis of pigmentation disorders of the skin (macroscopically, pigmentation was recognized only at 10–14 days after stimulation).
For clarifying whether the spectral changes observed in the above (Figure 4(b)) are specific for effects of reactive oxygen species, the time-dependent intensity changes of the remarkable Raman signals for the Caucasian skin type after the H2O2 stimulation (Figure 4(b)) were compared to those without the H2O2 stimulation (the control). We confirmed that the drastic changes in the Raman signals within 4-5 days for the stimulated Caucasian type were not observed in the control.
Let us here discuss the information obtained using the Raman confocal microscope to the live tissue analysis. The intensities of Raman bands were measured in the fixed focal volume given by the Raman confocal microscope, and the information obtained there is affected by many factors (superposition of many chemical reactions). Even in the situation it is possible to estimate changes in the concentrations for Raman active chemical species since the intensity of a Raman band is changed in a proportional manner to concentrations. In Figure 4(b), concerning to the Caucasian skin models, the remarkable Raman bands at 1455, 1662, and 1007 cm−1 gave intensity changes with synchronicity as function of time, whose bands correspond to the vibrations of the CH2, amide, and phenylalanine portions, respectively. The observation of the intensity changes with synchronicity suggests that the concentrations of the Raman active molecules in the fixed focal volume were changed in the same manner. It is probable that the observed dermal cells were changed to different states after the H2O2 stimulation to give the synchronous changes in the Raman bands.
In Figure 4(b), the 3D human skin models containing melanocytes exhibited different responses to H2O2. It is of interest that Caucasian keratinocytes commonly used in all the three skin-type models, the majority of the dermal cells, were influenced by the different types of the melanocytes present (the skin models are fabricated by spreading dermal cells on the collagen sheet with the approximate ratio of one melanocyte to twenty keratinocytes; we can model three types of the skin models by choosing Caucasian, Asian, and Black type melanocytes; within melanosomes of a melanocyte, melanin is synthesized and transformed into surrounding keratinocytes through dendrites of the melanocyte; the melanocytes remained in the basal layer while keratinocytes were proliferated upward in order to form the three dimensionally developed skin models with the basal layer, prickle cell layer, granular cell layer, and keratin layer.) Melanin is a pigment with a complex chemical structure. Two types of melanin coexist in almost all human beings, and their ratio determines an individual’s hair and skin color [22, 23]. One is eumelanin, which is brown to black in color, and the other is pheomelanin, yellow to red in color. These are probably the main compounds that cause differences in dermal cells in terms of their sensitivity to H2O2. Melanin is related to the photoprotection of the skin through its ability to absorb and scatter light [22, 23]. Another function of melanin is in the reduction or generation of ROS [22, 23]. While ROS reduction is induced by eumelanin, ROS production is done by pheomelanin [22, 23].
With H2O2 stimulation, the time-dependent Raman spectra of three kinds of skin models exhibited different responses. Changes in the Raman signals were observed at the early stage, compared with the macroscopic pigmentation after stimulation. The properties of the skin models were characterized using the Raman technique. Raman bands for the Caucasian skin model showed large intensity changes within 4-5 days of stimulation, compared to those for the Asian and Black skin model. Eventually, eumelanin and pheomelanin are considered to be the main compounds that differentiate skin properties in terms of their sensitivity to H2O2. The findings are important since the early stage Raman detections of the skin identities may allow us to classify disorders or diseases such as stains, freckles, and cancers of the skin in a newly started manner. Our research group is at present interested in measuring the Raman spectra of single melanocytes or keratinocytes, distinguishing the locations in the target cells to study more specific chemical reactions. Also, we are testing the physical properties of hollow fiber probes to measure Raman spectra of the human skin as it is. These will be discussed elsewhere in the near future.
- A. Nijssen, K. Maquelin, L. F. Santos et al., “Discriminating basal cell carcinoma from perilesional skin using high wave-number Raman spectroscopy,” Journal of Biomedical Optics, vol. 12, no. 3, Article ID 034004, 2007.
- M. Gniadecka, P. A. Philipsen, S. Sigurdsson et al., “Melanoma diagnosis by Raman spectroscopy and neural networks: structure alterations in proteins and lipids in intact cancer tissue,” Journal of Investigative Dermatology, vol. 122, no. 2, pp. 443–449, 2004.
- P. J. Caspers, G. W. Lucassen, and G. J. Puppels, “Combined in vivo confocal Raman spectroscopy and confocal microscopy of human skin,” Biophysical Journal, vol. 85, no. 1, pp. 572–580, 2003.
- J. R. Ferraro, K. Nakamoto, and C. B. Brown, Introductory Raman Spectroscopy, Elsevier, Amsterdam, The Netherlands, 2nd edition, 2003.
- N.-T. Yu, B. H. Jo, R. C. C. Chang, and J. D. Huber, “Single crystal Raman spectra of native insulin. Structures of insulin fibrils, glucagon fibrils, and intact calf lens,” Archives of Biochemistry and Biophysics, vol. 160, no. 2, pp. 614–622, 1974.
- N.-T. Yu and E. J. East, “Laser Raman spectroscopic studies of ocular lens and its isolated protein fractions,” Journal of Biological Chemistry, vol. 250, no. 6, pp. 2196–2202, 1975.
- E. J. East, R. C. C. Chang, and Nai-Teng Yu, “Raman spectroscopic measurement of total sulfhydryl in intact lens as affected by aging and ultraviolet irradiation. Deuterium exchange as a probe for accessible sulfhydryl in living tissue,” Journal of Biological Chemistry, vol. 253, no. 5, pp. 1436–1441, 1978.
- M. Delhaye and P. Dhamelincourt, “Raman microprobe and microscope with laser excitatio,” Journal of Raman Spectroscopy, vol. 3, no. 1, pp. 33–43, 1975.
- M. E. Andersen and R. Z. Muggll, “Microscopical techniques with the molecular optics laser examiner Raman microprobe,” Analytical Chemistry, vol. 53, no. 12, pp. 1772–1777, 1981.
- H. Ishida and A. Ishitani, “Raman microprobe analysis of thin films formed on the surface of silver electrical contacts utilizing the surface-enhanced raman scattering effect,” Applied Spectroscopy, vol. 37, no. 5, pp. 450–455, 1983.
- H. Ishida, R. Kamoto, S. Uchida et al., “Raman microprobe and fourier transform-infrared microsampling studies of the microstructure of gallstones,” Applied Spectroscopy, vol. 41, no. 3, pp. 407–412, 1987.
- Y. S. Huang, T. Karashima, M. Yamamoto, and H. O. Hamaguchi, “Molecular-level investigation of the structure, transformation, and bioactivity of single living fission yeast cells by time- and space-resolved Raman spectroscopy,” Biochemistry, vol. 44, no. 30, pp. 10009–10019, 2005.
- R. J. Swain, S. J. Kemp, P. Goldstraw, T. D. Tetley, and M. M. Stevens, “Assessment of cell line models of primary human cells by Raman spectral phenotyping,” Biophysical Journal, vol. 98, no. 8, pp. 1703–1711, 2010.
- H. P. Buschman, E. T. Marple, M. L. Wach et al., “In vivo determination of the molecular composition of artery wall by intravascular Raman spectroscopy,” Analytical Chemistry, vol. 72, no. 16, pp. 3771–3775, 2000.
- A. S. Haka, Z. Volynskaya, J. A. Gardecki et al., “In vivo margin assessment during partial mastectomy breast surgery using Raman spectroscopy,” Cancer Research, vol. 66, no. 6, pp. 3317–3322, 2006.
- Y. Komachi, H. Sato, Y. Matsuura, M. Miyagi, and H. Tashiro, “Raman probe using a single hollow waveguide,” Optics Letters, vol. 30, no. 21, pp. 2942–2944, 2005.
- T. Katagiri, Y. S. Yamamoto, Y. Ozaki, Y. Matsuura, and H. Sato, “High axial resolution raman probe made of a single hollow optical fiber,” Applied Spectroscopy, vol. 63, no. 1, pp. 103–107, 2009.
- Y. Komachi, H. Sato, K. Aizawa, and H. Tashiro, “Micro-optical fiber probe for use in an intravascular Raman endoscope,” Applied Optics, vol. 44, no. 22, pp. 4722–4732, 2005.
- Y. Hattori, Y. Komachi, T. Asakura et al., “In vivo Raman study of the living rat esophagus and stomach using a micro-Raman probe under an endoscope,” Applied Spectroscopy, vol. 61, no. 6, pp. 579–584, 2007.
- Z. Huang, H. Lui, X. K. Chen, A. Alajlan, D. I. McLean, and H. Zeng, “Raman spectroscopy of in vivo cutaneous melanin,” Journal of Biomedical Optics, vol. 9, no. 6, pp. 1198–1205, 2004.
- I. Notingher and L. L. Hench, “Raman microspectroscopy: a noninvasive tool for studies of individual living cells in vitro,” Expert Review of Medical Devices, vol. 3, no. 2, pp. 215–234, 2006.
- N. Agar and A. R. Young, “Melanogenesis: a photoprotective response to DNA damage?” Mutation Research, vol. 571, no. 1-2, pp. 121–132, 2005.
- S. Takeuchi, W. Zhang, K. Wakamatsu et al., “Melanin acts as a potent UVB photosensitizer to cause an atypical mode of cell death in murine skin,” Proceedings of the National Academy of Sciences of the United States of America, vol. 101, no. 42, pp. 15076–15081, 2004.