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J Dent Res 82(2): 141-145, 2003
© 2003 International and American Associations for Dental Research

RESEARCH REPORT
Biomaterials & Bioengineering

Hybridization Efficiency of the Adhesive/Dentin Interface with Wet Bonding

Y. Wang1, and P. Spencer1,2,*

1 Department of Oral Biology and
2 Department of Pediatric Dentistry, University of Missouri-Kansas City School of Dentistry, 650 E. 25th St., Kansas City, MO 64108;

*corresponding author, spencerp{at}umkc.edu


   ABSTRACT
TOP
 ABSTRACT
INTRODUCTION
 MATERIALS & METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Although it is generally proposed that dentin bonding results from adhesive infiltration of superficially demineralized dentin, it is not clear how well the resin monomers seal the dentin collagen fibrils under wet bonding conditions. The aim of this study was to determine the quality and molecular structure of adhesive/dentin (a/d) interfaces formed with wet bonding as compared with adhesive-infiltrated demineralized dentin (AIDD) produced under controlled conditions (optimum hybrid). From each extracted, unerupted human 3rd molar, one fraction was demineralized, dehydrated, and infiltrated with Single Bond (SB) adhesive under optimum conditions; the remaining, adjacent fraction was treated with SB by wet bonding. AIDD and a/d interface sections were stained with Goldner’s trichrome; corresponding sections were analyzed with micro-Raman spectroscopy. The histomorphologic and spectroscopic results suggest that, under wet bonding, the a/d interface is a porous collagen web infiltrated primarily by the hydrolytically unstable HEMA.

KEY WORDS: dentin • adhesive • spectroscopy • Raman • staining


   INTRODUCTION
TOP
 ABSTRACT
 INTRODUCTION
MATERIALS & METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
The durability of the adhesive/dentin (a/d) bond is directly related to the quality of the hybrid layer that connects the bulk adhesive to the subjacent, intact dentin. Ideally, the adhesive monomers occupy all the space that remains following removal of the mineral by acid-etching and envelop the exposed collagen fibrils (Pashley et al., 1993). Recent studies have shown that this objective is frequently not achieved (Sano et al., 1995; Spencer and Swafford, 1999; Spencer et al., 2000; Wang and Spencer, 2002a). Although these studies have contributed substantially to our understanding, they do not provide quantitative information on resin infiltration at the dentin interface as compared with an optimum hybrid layer (Nakabayashi and Pashley, 1997).

To understand the molecular process of adhesive monomer penetration, we used micro-Raman spectroscopy (µRS) and a novel microscopic staining technique to characterize adhesive-infiltrated demineralized dentin (AIDD) created under controlled conditions, i.e., the optimum hybrid layer, as compared with the a/d interface prepared by the wet-bonding technique. A current commercial one-bottle adhesive consisting of hydrophilic (HEMA) and hydrophobic (BisGMA) components was used for both the AIDD and a/d interface specimens. The quality of the a/d interface formed under wet bonding was determined quantitatively by comparison of the µRS and light microscopic results collected on the interface with the data acquired from the optimum hybrid layer. The null hypothesis was that adhesive resin applied under wet-bonding conditions envelops the exposed collagen fibrils, forming a structurally integrated hybrid layer at the molecular level.


   MATERIALS & METHODS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS & METHODS
RESULTS
 DISCUSSION
 REFERENCES
 
Preparation of Adhesive-infiltrated Demineralized Dentin (AIDD)
Six extracted unerupted human third molars stored at 4°C in 0.9% w/v NaCl containing 0.002% sodium azide were used. The teeth were collected after the patients’ informed consent was obtained under a protocol approved by the UMKC adult health sciences institutional review board. Using a water-cooled low-speed diamond saw (Buehler Ltd, Lake Bluff, IL, USA), we prepared dentin slabs (10 mm long, 2 mm high, and 1.5 mm wide) from these teeth. The adjacent fraction of the cut tooth was used for the a/d interface specimens. The dentin slabs were demineralized in 0.5 M EDTA (pH 7.3) at 25°C for 7 days; the solution was changed on alternate days. At the end of 1 wk, randomly selected dentin slabs were sectioned and Raman spectra acquired. The absence of spectral features associated with the mineral (P-O band at 960 cm-1) indicated complete demineralization. The demineralized specimens were rinsed thoroughly with distilled water.

The demineralized dentin slabs were dehydrated for 12 hrs in each of the following: 70, 95, 100% ethanol. Following dehydration, the specimens were immersed in Single Bond (SB) adhesive (3M, St. Paul, MN, USA). The demineralized dentin collagen/adhesive specimens were placed in the dark for 72 hrs. After 72 hrs, 3 specimens were polymerized with visible light (Spectrum light, Dentsply, Milford, DE, USA); the remaining 3 specimens were desiccated under vacuum for 24 hrs for further removal of any residual solvent prior to polymerization.

Preparation of the Adhesive/Dentin (a/d) Interface Specimen
The adhesive/dentin (a/d) specimen preparation has been detailed in previous publications (Spencer and Swafford, 1999; Spencer et al., 2000; Wang and Spencer, 2002a). For each of the 6 molars, we used the fraction of the cut tooth adjacent to the slab prepared for adhesive infiltration. We created a uniform smear layer by abrading with 600grit sandpaper under water cooling and treated the prepared dentin specimens with two consecutive layers of SB adhesive following the manufacturer’s instructions for wet bonding. After polymerization, the specimens were stored in water at 25°C for at least 24 hrs before further sectioning. The treated dentin surfaces were sectioned perpendicular and parallel to the bonded surface with a water-cooled low-speed diamond saw.

Differential Staining Technique
The rectangular, 10 x 2 x 1.5 mm, slabs of both Single Bond adhesive-infiltrated demineralized dentin (AIDD) and adhesive/dentin (a/d) interface specimens were mounted on a methacrylate support, and 3-µm-thick sections were cut from the face of the slab by means of a tungsten carbide knife mounted on a Polycut S "sledge" microtome. Following recovery of the microtomed sections, the remaining fraction of the AIDD and a/d interface slabs was used for micro-Raman spectroscopic analysis. Differential staining of the microtomed sections was accomplished with Goldner’s trichrome. Stained sections were dehydrated, cover-slipped, and examined under a Nikon E 800 light microscope.

Micro-Raman Spectroscopy
The micro-Raman spectrometer consisted of an argon ion laser beam (514.5 nm) focused through a X60 Olympus Plan Neofluor water-immersion objective (NA 1.2) to a ~ 1.5-µm beam diameter. Raman back-scattered light was collected through the objective and resolved with a monochromator. The spectra were recorded with a software-controlled CCD array. The laser power was approximately 3 mW; an imaging system and high-resolution monitor were incorporated to allow for visual identification of the position at which the Raman spectrum was obtained. Spectra were Raman-shift-frequency-calibrated with the use of known lines of neon and silicon.

Raman spectra of AIDD were acquired from a minimum of 6 different sites on each sample. Spectra were obtained at a resolution of ~ 6 cm-1 over the spectral region of 875-1785 cm-1 and with an integration time of 60 sec. A comparison of the spectra that were collected from the 6 different sites indicated complete overlap, suggesting homogeneous infiltration of adhesive throughout these samples.

Each a/d interface slab was placed at the focus of the objective and covered with distilled water in preparation for micro-Raman spectroscopic analysis. Spectra were acquired at positions corresponding to 1-µm intervals across the a/d interface with the use of the computer-controlled x-y-z stage with a minimum step width of 50 nm. Multiple sites across the interface of each specimen were examined spectroscopically. Overlap of the spectra from these sites confirmed the reproducibility of the technique. No post-processing of the data was performed.


   RESULTS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS & METHODS
 RESULTS
DISCUSSION
 REFERENCES
 
In the photomicrograph of a Goldner’s-trichrome-stained section of the a/d interface, the mineralized dentin is green, while the bulk adhesive appears as a very pale yellow (Fig. 1aGo). A distinct red region, representing exposed collagen at the a/d interface that was available for reaction with the Goldner’s trichrome stain, is visible in Fig. 1aGo. The pale-colored resin tags and dark red intertubular area in the a/d interface are clearly differentiated in this Fig. The mean width of the entire zone that showed red color distinct from either pure SB or mineralized dentin was 8 ± 0.6 µm. Representative photomicrographs of Goldner’s-trichrome-stained sections from the AIDD are shown in Figs. 1b and 1cGo. Fig. 1bGo shows a stained section recovered from the AIDD specimen which was polymerized before removal of ethanol solvent. The ~ 4-µm-diameter adhesive tags appeared clear, while the intertubular regions stained light orange. A section recovered from the AIDD with removal of ethanol did not pick up stain (Fig. 1cGo).



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  		Figure 1. Light micrographs and Raman spectra of Single Bond adhesive/dentin interface (a) and Single Bond adhesive-infiltrated demineralized dentin (AIDD) without or with removal of ethanol before polymerization (b, c, respectively). These 3-µm sections were stained with Goldner’s trichrome; corresponding Raman spectra were recorded from the intertubular area of the samples.

 
The corresponding Raman spectra of the intertubular region of the a/d interface and intertubular demineralized dentin collagen infiltrated with adhesive are also presented in Fig. 1Go. The bands associated with the adhesive occur at 1720 cm-1 (carbonyl), 1609 cm-1 (phenyl C=C), 1453 cm-1 (CH2 def), 1187 cm-1 (gem-dimethyl), and 1113 cm-1 (C-O-C), while the bands associated with collagen occur at 1667 cm-1 (amide I), 1454 cm-1 (CH2 def), and 1245 cm-1 (amide III). In comparing these spectra, we saw that the bands associated with adhesive are dominant in the AIDD specimens, while the features associated with collagen dominate the spectrum recorded from the a/d interface. The difference in the relative ratios of the Raman features of collagen and adhesive in the AIDD specimens with and without removal of ethanol is small. In comparing spectra from the AIDD with those recorded from the a/d interface, we noted that the reduced relative intensity of the adhesive bands (1113, 1187, 1609, 1720 cm-1) indicates less diffusion of resin monomers into the zone of demineralized dentin at the a/d interface.

Using a water immersion lens, we imaged the same slabs that were analyzed by light microscopy and acquired Raman spectra at 1-µm intervals across the a/d interface (Fig. 2aGo). As shown in Fig. 2bGo, in the micro-Raman mapping spectra collected from this a/d interface, the first spectrum was acquired from pure adhesive. Bands associated with the adhesive and collagen components of dentin are noted in the second spectrum. The Raman band of the P-O group (960 cm-1) in the tenth spectrum suggests that this represents the bottom of the demineralized dentin layer. Dentin was demineralized to a depth of ~ 7 µm, and the depth of partially demineralized dentin was ~ 3 µm (Fig. 2bGo). The spectra recorded at the 2nd, 4th, and 6th micrometer positions of the a/d interface are presented in detail, and major spectral changes have been marked with arrows (Fig. 2cGo). The decreased intensity of the Raman bands attributed to the adhesive (1113, 1187, 1454, 1609, 1720 cm-1) as a function of depth indicates the gradual decrease of adhesive infiltration into the demineralized dentin.



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  		Figure 2. Light micrograph (a) and corresponding Raman mapping spectra (b) acquired at 1-µm intervals across the Single Bond adhesive/dentin interface. The spectra marked with arrows (c) were recorded from sites corresponding to the demarcations noted on the light micrograph.

 
To determine the differences in composition of AIDD and the a/d interface at different depths, we calculated the ratios of the relative integrated intensities of bands associated with adhesive and the band associated with collagen (amide I) (TableGo). The composition of SB is 60-70 wt% BisGMA and 40-30 wt% HEMA (Spencer and Wang, 2002). The band at 1454 cm-1, which is assigned to the CH2 group of both BisGMA and HEMA, and the band at 1113 cm-1, which is assigned to the C-O-C group of BisGMA, were selected as measures of resin adhesive and BisGMA monomer, respectively. As listed in the TableGo, the mean ratios of 1454 cm-1/1667 cm-1 and 1113 cm-1/1667 cm-1 for AIDD are 0.927 and 0.60. These ratios are 0.913 and 0.41 for the a/d interface at the first micrometer, and decrease to 0.162 and 0.052, respectively, at the depth of the demineralized dentin. Fig. 3 (a,bGo) shows these relative ratios as a function of spatial position across the a/d interface. These ratios for AIDD are also shown in Fig. 3 (a,bGo ). As compared with the ratios for AIDD, the difference in the ratios of 1454/1667 and 1113/1667 of the a/d interface increased as a function of position, indicating less diffusion of resin monomers across the interface. The ratio of 1454/1667 shows a gradual decline, while the ratio of 1113/1667 (BisGMA/collagen) shows a dramatic decrease in the concentration of BisGMA monomer across the a/d interface.


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  		Table. The Raman Intensity Ratios and Percent of Monomer Penetration
 


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  		Figure 3. Raman intensity ratios of 1454/1667 (a) and 1113/1667 (b) and penetration of BisGMA monomer and BisGMA/HEMA (c) as a function of spatial position across the adhesive/dentin interface. The comparable relative ratios calculated from the AIDD represent the optimum hybrid and are presented for comparison.

 
To quantify the penetration of the adhesive resin monomers, based on the results presented in the Table Goand Fig. 3 (a,bGo), we defined the AIDD prepared under controlled conditions as an optimum hybrid, which has 100% adhesive infiltration. A comparison of the penetration of BisGMA monomer and BisGMA/HEMA resin as a function of position across the a/d interface is presented in Fig. 3cGo and the TableGo. This comparison provided a quantitative representation of the percent of adhesive monomer penetration as a function of position. It was shown that ~ 98% resin monomers penetrated the first micrometer of the interface, but only ~ 68% BisGMA monomer penetrated the first micrometer of demineralized dentin. The percent of the BisGMA/HEMA resin monomers penetrating the demineralized dentin drops gradually from ~ 89% at the second micrometer to ~ 71% at the third micrometer, and at the depth of the demineralized dentin (~ 8 µm), the percent of BisGMA/HEMA resin monomers is ~ 18%. In comparison, the percent of BisGMA monomer dropped very rapidly, from ~ 42% at the second micrometer to ~ 32% at the third micrometer; from this position to the bottom of the demineralized zone of dentin, the percent of BisGMA penetration is only ~ 8% as compared with the optimum hybrid.


   DISCUSSION
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS & METHODS
 RESULTS
 DISCUSSION
REFERENCES
 
Dentin can be regarded as a biological composite with organic and inorganic components (Marshall et al., 1997). After extraction of the inorganic or mineral component, the voids can be infiltrated with resin, thus forming a new composite made up of resin matrix filled with a fibrous collagen. This new structure is a hybrid of resin and collagen (Nakabayashi, 1992). As shown in Fig. 1Go, this optimum hybrid structure was achieved when adhesive resin infiltrated dehydrated, demineralized dentin prepared under controlled conditions (Fig. 1cGo), but not at the a/d interface formed by the wet-bonding technique. By use of the histomorphologic technique described here, any collagen that is not encased in adhesive resin is available for reaction with the Goldner’s trichrome stain (Spencer and Swafford, 1999; Spencer et al., 2000). The section of AIDD specimen without total removal of ethanol solvent stains slightly. The distinct red zone at the a/d interface (Fig. 1aGo) indicated that the adhesive did not encapsulate the collagen fibrils throughout the width of the demineralized dentin. This novel staining technique, which identifies exposed collagenous protein at the light microscopic level, provides a unique, clear representation of the extent and degree to which the adhesive resins envelop the collagen fibrils of the demineralized dentin matrix.

Corresponding Raman spectra recorded from the intertubular area of the a/d interface and the AIDD sections confirmed the above observation. The lower adhesive contribution in the spectrum of the a/d interface, as compared with the AIDD, indicates limited diffusion of resin monomers into the wet demineralized dentin. Gradual decreases in intensity of Raman bands associated with adhesive have been reported by previous authors (Van Meerbeek et al., 1993; Hashimoto et al., 2002). However, in these studies, the authors measured the amount of resin penetration based on the absolute intensity of adhesive bands (Hashimoto et al., 2002), totally ignoring the collagen matrix, the key component of acid-etched dentin. The absolute intensity of back-scattering Raman band is dramatically affected by many factors, including the smoothness of the sample surface, position of focusing, depth of detection, fluorescence of biological components, and stability of the instrument and laser power (Walton, 1970; Chase, 1991). Since it is very difficult to maintain all of these conditions the same across the breadth of the sample, the band intensity may vary from one measurement to the next, even at the same spot on the sample. To account for the effects of instrumental fluctuation and errors, we used the Raman band associated with the collagen matrix as an internal standard throughout our studies (Spencer et al., 2000, 2001; Wang and Spencer, 2002a,b).

Although there is substantial evidence to suggest that the resin-dentin interdiffusion zone is porous (Sano et al., 1994, 1995; Tay et al., 1995), there is no technique available to measure the extent of adhesive infiltration at the a/d interface and to determine how adhesive penetration at the interface relates to the condition of complete infiltration. In our previous studies (Spencer et al., 2000; Wang and Spencer, 2002a), the weight percent of adhesive at each micrometer as a function of spatial position across the a/d interface was determined. To facilitate the comparison of adhesive penetration across the breadth of the interface, we assumed that the adhesive fully penetrated the first micrometer of the a/d interface. However, to fully identify, characterize, and understand the weak links in the a/d bond, it is important for us to know if the adhesive occupied all the space left by the mineral after acid-etching. A new method which truly calculates the extent of adhesive penetration at the a/d interface as compared with optimum hybrid specimens was proposed in this study. At the first micrometer of the a/d interface, only ~ 68% of the concentration of BisGMA in the original adhesive penetrated the demineralized dentin (Fig. 3cGo). In comparison, the resin components (including HEMA) diffused more readily into the demineralized dentin zone than the BisGMA component.

In summary, this study demonstrates the advantages of using molecular microanalysis in conjunction with a novel histomorphologic technique to study the impact of wet bonding on the development of an ideal dentin/adhesive bond. It represents a clear, quantitative method for determining the quality of the hybrid layer. The results suggest that, under wet bonding, the a/d interface is not an impervious collagen/polymer network but a porous web; the composition of this web is predominantly collagen and HEMA, with a lesser contribution from the BisGMA component. The null hypothesis was rejected. The results of this study suggest that the critical dimethacrylate component (BisGMA), which contributes the most to the crosslinked polymeric adhesive, infiltrates a fraction of the total wet demineralized, intertubular dentin layer.


   ACKNOWLEDGMENTS
 
This investigation was supported by USPHS Research Grant DE 12487 from the National Institute of Dental and Craniofacial Research, National Institutes of Health, Bethesda, MD 20892. The authors gratefully acknowledge 3M, Dental Products Division, for donating the dentin adhesive products used in this study. A preliminary report was presented at the 2002 meeting of the International and American Associations for Dental Research, San Diego, CA, USA.

Received April 19, 2002; Last revision August 29, 2002; Accepted November 5, 2002


   REFERENCES
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS & METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Chase DB (1991). Modern Raman instrumentation and techniques. In: Analytical Raman spectroscopy. Grasselli JG, Bulkin BJ, editors. New York: John Wiley & Sons, Inc., pp. 21-43.

Hashimoto M, Ohno H, Kaga M, Sano H, Endo K, Oguchi H (2002). The extent to which resin can infiltrate dentin by acetone-based adhesives. J Dent Res 81:74–78.[Abstract/Free Full Text]

Marshall GW Jr, Marshall SJ, Kinney JH, Balooch M (1997). The dentin substrate: structure and properties related to bonding. J Dent 25:441–458.[ISI][Medline]

Nakabayashi N (1992). The hybrid layer: a resin-dentin composite. Proc Finn Dent Soc 88(Suppl 1):321–329.

Nakabayashi N, Pashley DH (1997). Hybridization of dental hard tissues. Tokyo: Quintessence Publishing Co., Ltd.

Pashley DH, Ciucchi B, Sano H, Homer JA (1993). Permeability of dentin to adhesive agents. Quintessence Int 24:618–631.[Medline]

Sano H, Shono T, Takatsu T, Hosoda H (1994). Microporous dentin zone beneath resin-impregnated layer. Oper Dent 19:59–64.[ISI][Medline]

Sano H, Takatsu T, Ciucchi B, Horner JA, Matthews WG, Pashley DH (1995). Nanoleakage: leakage within the hybrid layer. Oper Dent 20:18–25.[ISI][Medline]

Spencer P, Swafford JR (1999). Unprotected protein at the dentin-adhesive interface. Quintessence Int 30:501–507.[ISI][Medline]

Spencer P, Wang Y (2002). Adhesive phase separation at the dentin interface under wet bonding conditions. J Biomed Mater Res 62:447–456.[ISI][Medline]

Spencer P, Wang Y, Walker MP, Wieliczka DM, Swafford JR (2000). Interfacial chemistry of the dentin/adhesive bond. J Dent Res 79:1458–1463.[Abstract/Free Full Text]

Spencer P, Wang Y, Walker MP, Swafford JR (2001). Molecular structure of acidetched dentin smear layers—in situ study. J Dent Res 80:1802–1807.[Abstract/Free Full Text]

Tay FR, Gwinnett AJ, Pang KM, Wei SH (1995). Variability in microleakage observed in a total-etch wet-bonding technique under different handling conditions. J Dent Res 74:1168–1178.[Abstract/Free Full Text]

Van Meerbeek B, Mohrbacher H, Celis JP, Roos JR, Braem M, Lambrechts P, et al. (1993). Chemical characterization of the resin-dentin interface by micro-Raman spectroscopy. J Dent Res 72:1423–1428.[Abstract/Free Full Text]

Walton AG, Deveney MJ, Koenig JL (1970). Raman spectroscopy of calcified tissue. Calcif Tissue Res 6:162–167.[ISI][Medline]

Wang Y, Spencer P (2002a). Quantifying adhesive penetration in adhesive/dentin interface using confocal Raman microspectroscopy. J Biomed Mater Res 59:46–55.[ISI][Medline]

Wang Y, Spencer P (2002b). Analysis of acid-treated dentin smear debris and smear layers using confocal Raman microspectroscopy. J Biomed Mater Res 60:300–308.[ISI][Medline]




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