Front. Physiol. Frontiers in Physiology Front. Physiol. 1664-042X Frontiers Media S.A. 10.3389/fphys.2017.00307 Physiology Original Research Deletion of Slc26a1 and Slc26a7 Delays Enamel Mineralization in Mice Yin Kaifeng 1 2 Guo Jing 3 Lin Wenting 1 Robertson Sarah Y. T. 1 Soleimani Manoocher 4 Paine Michael L. 1 * 1Center for Craniofacial Molecular Biology, Herman Ostrow School of Dentistry of University of Southern California Los Angeles, CA, USA 2Department of Orthodontics, Herman Ostrow School of Dentistry of University of Southern California Los Angeles, CA, USA 3Department of Endodontics, Herman Ostrow School of Dentistry of University of Southern California Los Angeles, CA, USA 4Department of Medicine, University of Cincinnati, Research Services, Veterans Affairs Medical Center Cincinnati, OH, USA

Edited by: Steven Joseph Brookes, Leeds Dental Institute, UK

Reviewed by: Eric Everett, University of North Carolina at Chapel Hill, USA; Pamela DenBesten, University of California, San Francisco, USA

*Correspondence: Michael L. Paine paine@usc.edu

This article was submitted to Craniofacial Biology and Dental Research, a section of the journal Frontiers in Physiology

 16 05 2017 2017 8 307 16 03 2017 28 04 2017 Copyright © 2017 Yin, Guo, Lin, Robertson, Soleimani and Paine. 2017 Yin, Guo, Lin, Robertson, Soleimani and Paine

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Amelogenesis features two major developmental stages—secretory and maturation. During maturation stage, hydroxyapatite deposition and matrix turnover require delicate pH regulatory mechanisms mediated by multiple ion transporters. Several members of the Slc26 gene family (Slc26a1, Slc26a3, Slc26a4, Slc26a6, and Slc26a7), which exhibit bicarbonate transport activities, have been suggested by previous studies to be involved in maturation-stage amelogenesis, especially the key process of pH regulation. However, details regarding the functional role of these genes in enamel formation are yet to be clarified, as none of the separate mutant animal lines demonstrates any discernible enamel defects. Continuing with our previous investigation of Slc26a1−/− and Slc26a7−/− animal models, we generated a double-mutant animal line with the absence of both Slc26a1 and Slc26a7. We showed in the present study that the double-mutant enamel density was significantly lower in the regions that represent late maturation-, maturation- and secretory-stage enamel development in wild-type mandibular incisors. However, the “maturation” and “secretory” enamel microstructures in double-mutant animals resembled those observed in wild-type secretory and/or pre-secretory stages. Elemental composition analysis revealed a lack of mineral deposition and an accumulation of carbon and chloride in double-mutant enamel. Deletion of Slc26a1 and Slc26a7 did not affect the stage-specific morphology of the enamel organ. Finally, compensatory expression of pH regulator genes and ion transporters was detected in maturation-stage enamel organs of double-mutant animals when compared to wild-type. Combined with the findings from our previous study, these data indicate the involvement of SLC26A1and SLC26A7 as key ion transporters in the pH regulatory network during enamel maturation.

 amelogenesis enamel maturation pH regulation bicarbonate transport SLC26a1 SLC26A7 DE019629 DE024724 DE021982 National Institutes of Health10.13039/100000002 Introduction

Acid-base balance is one of the major essential processes during amelogenesis (Simmer and Fincham, 1995; Smith et al., 1996; Smith and Nanci, 1996; Lacruz et al., 2010a, 2012b), and it has been suggested that fluctuations in extracellular pH level during maturation-stage enamel development are essential for mineral growth (Simmer and Fincham, 1995). Digestion of enamel matrix proteins (EMPs) through the endosome/lysosome pathway, following trafficking from the enamel space, relies highly on the acidic intracellular luminal environment (Lloyd, 1996). Previous studies have identified the functional role of several groups of genes, including carbonic anhydrases (Lezot et al., 2008), cystic fibrosis transmembrane conductance regulator (CFTR), chloride channels (CLCNs), solute carrier gene family 4 (SLC4s) and solute carrier gene family 9 (SLC9s), in maintaining the ameloblast-mediated pH homeostasis within both extracellular space and intracellular lumens (Dogterom and Bronckers, 1983; Lin et al., 1994; Wright et al., 1996a,b; Arquitt et al., 2002; Lyaruu et al., 2008; Paine et al., 2008; Bronckers et al., 2009, 2010; Josephsen et al., 2010; Wang et al., 2010; Lacruz et al., 2010a,b, 2012c, 2013a; Chang et al., 2011; Duan et al., 2011; Duan, 2014; Jalali et al., 2014; Reibring et al., 2014; Wen et al., 2014).

The solute carrier (SLC) 26A gene family encodes multiple anion transporters with chloride/bicarbonate exchanger activities (Xie et al., 2002; Petrovic et al., 2003a,b, 2004; Alper and Sharma, 2013). Animal models with mutations of Slc26a1, Slc26a6, and Slc26a7 exhibit disorders featuring disruption of ion homeostasis, such as urolithiasis, hepatotoxicity, renal tubular acidosis and impaired gastric secretion (Freel et al., 2006; Jiang et al., 2006; Xu et al., 2009; Dawson et al., 2010). Based on our previous study and those of Bronckers et al., Slc26a1/Sat1, Slc26a3/Dra, Slc26a4/pendrin, Slc26a6/Pat1 and Slc26a7/Sut1 are immunolocalized in secretory- and maturation-stage ameloblasts (Bronckers et al., 2011; Jalali et al., 2015; Yin et al., 2015). In particular, these genes mainly localize to the apical membrane/subapical vesicles of maturation ameloblast. In addition, the expression of Slc26a1, Slc26a6, and Slc26a7 is significantly upregulated at both RNA and protein levels during maturation stage compared to secretory stage (Yin et al., 2014, 2015). These are strong indications of the functional involvement of the Slc26 gene family in pH regulation during amelogenesis. However, the deletion of these genes individually fails to induce any abnormal enamel phenotypes, likely due to the compensatory expression of other pH regulatory genes and Slc26a isoforms, suggesting a yet-to-be-identified master pH response regulatory mechanism in amelogenesis (Bronckers et al., 2011; Jalali et al., 2015; Yin et al., 2015).

In this study, we generated an animal model with the absence of both Slc26a1 and Slc26a7 by breeding homozygous parents (Slc26a1−/− and Slc26a7−/−). We showed that the double-null enamel density was significantly lower in the regions that represent late maturation-, maturation-, and secretory-stage enamel development in wild-type mandibular incisors. However, the “maturation” and “secretory” enamel microstructures in double-mutant animals resembled those observed in wild-type secretory and/or pre-secretory stages. Elemental composition analysis revealed a lack of mineral deposition and an accumulation of carbon and chloride in double-mutant enamel, although absence of Slc26a1 and Slc26a7 did not affect the stage-specific morphology of the enamel organ including ameloblasts. Finally, compensatory expression of pH regulators and ion transporters at RNA level was detected in maturation-stage enamel organs of double-mutant animals. Taken together, the data obtained from double mutant animals (Slc26a1−/− and Slc26a7−/−) provide new evidence from a functional perspective to support the hypothesis that SLC26A1/SAT1 and SLC26A7/SUT1 are actively involved in ameloblast-mediated pH regulation during maturation-stage amelogenesis.

 Materials and methods Animals

All vertebrate animal manipulation was carried out in accordance with Institutional and Federal guidelines. The animal protocols were approved by the Institutional Animal Care and Use Committee at the University of Southern California (Protocol # 11736). For immunofluorescence analysis, we dissected mandibles and kidneys from rats (Wistar Hannover, 4-week, 100–110 g). Slc26a1+/− mice were purchased from the Jackson Laboratory (stock # 012892) and Slc26a7+/− mice were a kind gift from Dr. Manoocher Soleimani (Xu et al., 2009; Dawson et al., 2010). Slc26a1−/− and Slc26a7−/− mice were generated by breeding heterozygous (Slc26a1+/− or Slc26a7+/−) parents. To generate double-mutant animals with the absence of Slc26a1 and Slc26a7, we crossed Slc26a1−/− and Slc26a7−/− mice. The double-mutant lines were genotyped by PCR using primers designed in earlier studies (Xu et al., 2009; Dawson et al., 2010).

 Immunofluorescence

The expression patterns of Slc26a1 and Slc26a7 in maturation-stage ameloblasts were shown by co-localization using immunofluorescence (IF). Hemi-mandibles and kidneys obtained from Wistar Hannover rats (100–110 g body weight, 4 weeks old) were fixed in 4% paraformaldehyde (PFA) at 4°C overnight. The hemi-mandibles were then decalcified in 10% EDTA (pH 7.4) for 2 months. Sagittal sections were prepared from paraffin-embedded tissue blocks with a thickness of 7 μm. After being dewaxed, rehydrated and blocked by 1% bovine serum albumin (BSA) in PBST (1X, pH 7.4), the tissue sections were incubated with primary antibodies against Slc26a1 (Santa Cruz Biotechnology, Catalog # sc-132090, dilution 1:400) and Slc26a7 (Abcam, Catalog # ab65367, dilution 1:300). All tissue sections were stained with DAPI (Vector Laboratories; Catalog # H-1200) before cover slides were applied.

 μCT analysis

Mandibles were dissected from 4-week-old double-mutant animals and their age-matched wild-type controls. Samples from 12 animals in each group were prepared for μCT analysis (n = 12, SkyScan 1174) with the scanner setting to 50 kVp, 800 μA, and 6.7 μm resolution. The reconstruction and calculation of the enamel density of mandibular incisors and first molars were performed with Amira 3D Visualization and Analysis Software 5.4.3 (FEI Visualization Science Group, Burlington, MA, USA) (Wen et al., 2015). The potential statistical differences in the relative enamel density between double-mutant and wild-type groups were evaluated by a two-tailed Student's t-test using IBM SPSS Statistics 22.0 (significance level defined as P < 0.05).

 Scanning electron microscopy and energy-dispersive X-ray spectroscopy (EDS)

The hemi-mandibles prepared for μCT analysis (n = 12) were used for the subsequent SEM and EDS analyses. The samples were scanned and imaged by SEM and EDS according to previously published protocols (Lacruz et al., 2010b; Wen et al., 2014; Yin et al., 2015).

 Hematoxylin and eosin (H & E) staining

Mandibles were dissected from 4-week-old double-mutant animals and wild-type controls for H & E staining. The protocols followed those described in a previous study (Lacruz et al., 2012a).

 Realtime PCR analysis

RNA samples of maturation-stage enamel organs were extracted from mandibles of double-mutant and wild-type animals (n = 6) using a method described previously (Yin et al., 2015). cDNA used for real-time PCR analysis was prepared using the miScript II RT Kit with miScript HiFlex Buffer (Qiagen). To detect the expression changes in the genes that have been identified to be involved in maturation-stage pH regulation (Dogterom and Bronckers, 1983; Wright et al., 1996a,b; Andrejewski et al., 1999; Arquitt et al., 2002; Lyaruu et al., 2008; Paine et al., 2008; Bertrand et al., 2009; Bronckers et al., 2009, 2010, 2011; Josephsen et al., 2010; Wang et al., 2010; Lacruz et al., 2010a,b, 2011, 2012b,c, 2013b; Chang et al., 2011; Duan, 2014; Jalali et al., 2014; Yin et al., 2014, 2015), real-time PCR reactions were performed on a CFX96 TouchTM Real-Time PCR Detection System (Bio-rad Life Sciences) with iQ SYBR® Green supermix (Bio-rad Life Science) and mouse-specific primers (Table 1). The Ct values were normalized to those of Actb (Beta-actin). The ΔΔCt method was used to calculate the fold changes in gene expression (double-mutant relative to wild-type; Livak and Schmittgen, 2001; Schmittgen and Livak, 2008). Two-tailed Student's t-tests were used to detect the potential differences in the expression levels of gene transcripts between double-mutant and wild-type groups (significance level defined as P < 0.05). Data were analyzed using IBM SPSS Statistics 22.0 software.

Mouse-specific primers for qPCR.

Symbol Accession Region Forward (5′–3′) Reverse (5′–3′)
Car2 NM_009801 4–173 TCCCACCACTGGGGATACAG CTCTTGGACGCAGCTTTATCATA
Car6 NM_009802 61–160 TGGAGCTATTCAGGGGATGATG CCGTCTTCACGTCGATGGG
Cftr NM_021050 957–1,132 GCATATTGTTGGGAATCAGC ACGATTCCGTTGATGACTGT
Ae2 NM_009207 3,282–3,523 CATGGAGACACAGATCACCA GCTGTTCCTTGACTTCCTGA
Ae4 NM_172830 10-127 CCAGGGCAGGGGGATTTTG CCCCAATGTCTATGCCTGAGG
NBCe1 NM_018760 246–489 CTCCGAGAACTACTCCGACA ACCCTGCTCCACTTTCTCTT
Slc26a6 NM_134420 2,023–2,184 TTGCTGGAGCTGTATCTTCC TGTTTGCCTTCCAAAGAGAG
Lamp1 NM_010684 930–1,076 TCTATGGCACTGCAACTGAA GGCTCTGTTCTTGTTCTCCA
Lamp2 NM_001017959 785–916 AACTTCAACACCCACTCCAA AAAGGCACCTTCTCCTCAGT
Lamp3 NM_007653 598–809 CACAGACTGGGAAAACATCC TAATTCCCAAGACCTCCACA
Lamp4 NM_009853 630–811 ACATCAGAGCCCGAGTACAG GGTGAACAGCTGGAGAAAGA
Clcn7 NM_011930 316–477 CCAAGGAGATTCCACACAAC CAATGAGGGCACAGATAACC
Rab21 NM_024454 723–963 TCCGCTAAACAGAACAAAGG GGCAATGATCCACAGTTCTC
Alpl NM_007431 2,228–2,472 TCTGCTCAGGATGAGACTCC TCCCTTTTAACCAACACCAA
Nhe1 NM_016981.2 780–972 CATCCTTGTCTTCGGGGAGTC GGAGGTGAAAGCTGCGATTAC
Actb NM_007393 792–951 AAGAGCTATGAGCTGCCTGA TACGGATGTCAACGTCACAC
Results SLC26A1 and SLC26A7 do not colocalize in maturation-stage ameloblasts

We revisited the expression patterns of SLC26A1 and SLC26A7 in rodent maturation-stage ameloblasts by conducting colocalization analysis using immunofluorescence. The expression of Slc26a1 was mainly immunolocalized to the apical membrane of maturation ameloblast (Figure 1A). In contrast, SLC26A7 showed more expression in the cytoplasmic area in addition to an apical/subapical distribution (Figure 1A). No apparent overlaps in fluorescence signals from SLC26A1 and SLC26A7 were observed (Figure 1A). Tissue sections prepared from rat kidneys were stained with the same antibodies as a reference (Figure 1B).

Colocalization analysis of Slc26a1 with Slc26a7. ES, Enamel space; Am, Ameloblast; PL, Papillary layer; CT, Connective tissue. (A) Colocalization of SLC26A1and SLC26A7 in maturation-stage ameloblasts by confocal microscopy at 63x magnification. SLC26A1 immunolocalized to the apical membrane of maturation-stage ameloblasts. SLC26A7 showed more expression in the cytoplasmic area in addition to an apical/subapical distribution. Apparent overlaps in fluorescence from SLC26A1 and SLC26A7 were not observed. (B) Tissue sections prepared from rat kidneys were stained with the same antibodies as a reference. All sections were counterstained with DAPI to highlight the nuclei (blue).

 Double-mutant mandibular incisors demonstrate decreased enamel density

We dissected hemi-mandibles from 4-week-old double-mutant animals and their age-matched wild-type controls for μCT analysis. After 3D reconstruction from raw dicom files, we selected three regions to analyze the enamel density of incisors, which were indicated by the three reference planes along the long axis of the mandibular incisors (Figure 2). The first reference plane was placed at the region where bony support ends (Figures 2A3,B3). The second and the third reference planes sectioned though the first and the third mandibular molars (Figures 2A5,A7,B5,B7). The three reference planes from anterior to posterior represent late-maturation, maturation and secretory stages, respectively (Nanci, 2008; Lacruz et al., 2011, 2012b; Yin et al., 2014, 2015). In a 4-week-old wild-type mouse, the enamel of the mandibular incisor is fully mature (maturation-stage) between the first and the second reference planes (Figures 2A2–A6) (Yin et al., 2015). In contrast, the double-mutant enamel at the first and second reference planes showed statistically significant decreases in relative density (Figures 2B2–B6, 3A,B, P < 0.05). The double-mutant enamel density was approximately 14.3% lower than wild-type enamel density at the first reference plane (Figure 3A). At the second reference plane, the density gap between double-mutant and wild-type enamel was even higher—35.7% (Figure 3B). The enamel on mandibular incisors at the third reference plane is in secretory stage in wild-type animals (Yin et al., 2015), and the difference in relative enamel density of incisors was not statistically significant between wild-type and double-mutant groups (Figures 2A8,B8, 3C).

μCT analysis of wild-type and double-mutant mandibular incisors. (A1) Wild-type semi-mandible. (A2) Wild-type incisor viewed from the labial surface. (B1) Double-mutant semi-mandible. (B2) Double-mutant incisor viewed from the labial surface. We selected three regions to analyze the enamel density of incisors, which are indicated by the three reference planes along the long axis of mandibular incisors. The first reference plane was placed at the region where bony support begins (A3,B3). The second and the third reference planes sectioned though the first (A5,B5) and the third mandibular molars (A7,B7). In the wild-type sample, the three reference planes from anterior to posterior represent late maturation, maturation and secretory stages, respectively. (A4,A6,A8,B4,B6,B8) Are cross-sectional views of the regions of the three reference planes. Colors varying from blue to red in (A1–A3,A5,A7,B1–B3,B5,B7) indicate an increase in density. The area of mandibular incisor enamel is labeled by * in (A4,A6,A8,B4,B6,B8).

Quantification of enamel density in wild-type and double-mutant mandibular incisors. WT, Wild-type; DM, Double-mutant. (A) At the first reference plane, the double-mutant enamel density was approximately 14.3% lower than that of wild-type enamel (P = 0.015). (B) At the second reference plane, the density gap between double-mutant and wild-type enamel was even higher—35.7% (P = 0.010). (C) The difference in relative enamel density of mandibular incisors was not significant between the wild-type and double-mutant groups (P = 0.56). *P < 0.05.

Based on μCT analysis, we also quantified the relative density of mandibular first molars. For calculating the enamel density of each molar, we averaged the measurements obtained from mesial, middle and distal cusps (Figure 4). Although the double-mutant molars demonstrated lower enamel density than wild-type molars, the differences were not statistically significant (Figure 4C, P = 0.35).

Quantification of enamel density in wild-type and double-mutant mandibular first molars. WT, Wild-type; DM, Double-mutant. (A1–A3) Cross-sectional views of wild-type hemi-mandible at reference planes 1, 2 and 3. (B1–B3) Cross-sectional views of double-mutant hemi-mandible at reference planes 1, 2, and 3. (C) We averaged the measurements obtained from mesial, middle and distal cusps (reference planes 1, 2, and 3). The double-mutant molars demonstrated lower enamel density than wild-type molars, but the difference was not statistically significant (P = 0.35).

 Absence of <italic>Slc26a1</italic> and <italic>Slc26a7</italic> disrupts development of enamel microstructure

For SEM analysis, we used the same reference planes as in the μCT analysis (Figures 2, 5). We exposed the surface of interest by fracturing the mandibular incisors in the coronal direction, which was consistent with the orientation of the reference planes. At the first and the second reference planes, wild-type enamel showed typical microstructure of maturation-stage enamel with rods and interrods laid out in a decussating and orderly pattern (Figures 5A1,A1',B1,B1'). In wild-type enamel at secretory stage, which was marked by the third reference plane, enamel rods did not reach full thickness and the boundary between rod and interrod structure was not yet well defined (Figures 5C1,C1). In comparison, the structure of double-mutant enamel at the first and the second reference planes was similar to that observed at the second and the third reference planes in wild-type group, respectively (Figures 5A2,A2',B2,B2'), suggesting the double knockout animals showed a delay in maturation. Furthermore, there was a complete lack of decussating pattern in double-mutant enamel in the region labeled by the third reference plane, and aprismatic enamel/enamel-like structure dominated the whole vision field (Figures 5C2,C2′).

SEM analysis of enamel microstructures in wild-type and double-mutant mandibular incisors. WT, Wild-type; DT, Double-mutant. (A1–C1) Wild-type enamel at reference planes A, B, and C under 1000x magnification. (A1'–C1') The areas in (A1–B1) labeled with dotted frames under 5000x magnification. (A2–C2) Double-mutant enamel at the reference planes A, B, and C under 1000x magnification. (A2'–C2') The areas in (A2–B2) labeled with dotted frames under 5000x magnification. At the first and the second reference planes, wild-type enamel showed typical microstructure of maturation-stage enamel with rods and interrods laid out in a decussating and orderly pattern (A1,A1',B1,B1). In wild-type enamel at secretory stage, marked by the third reference plane, enamel rods did not reach full thickness and the boundary between rod and interrod structure was not yet well defined (C1,C1). In comparison, the structure of double-mutant enamel at the first and the second reference planes was similar to that observed at the second and the third reference planes, respectively, in the wild-type group (A2,A2,B2,B2). There was a complete lack of decussating pattern in double-mutant enamel in the region labeled by the third reference plane, and aprismatic enamel/enamel-like structure dominated the whole vision field (C2,C2).

 Double mutations impact mineral deposition

Following SEM, we analyzed the elemental compositions using EDS on the same regions of mandibular incisor enamel marked by the three previously mentioned reference planes (Figures 2, 5). At the first reference plane, there were no statistically significant differences between wild-type and double-mutant enamel in the atomic percentages (At%) of all the elements analyzed—Ca, P, O, C, Cl, Na, and Mg (Figures 6A1–A3). At the second reference plane, statistically significant changes were detected in the At% of Ca, P, C, and Cl (Figures 6B1–B3). The At% of Ca and P in double-mutant enamel decreased by ~26.7 and ~35.1%, respectively, compared to those in wild-type enamel (Figures 6B1–B3), while there were increases in the At% of C and Cl—~268.4 and ~18.6%, respectively (double-mutant/wild-type, Figures 6B1–B3). Changes in the elemental compositions at the third reference plane showed similar trends to those detected at the second reference plane—double-mutant enamel showed significantly lower At% of Ca, P, O, Mg (~92.8, ~69.2, ~29.6, and ~57.9%, Figures 6B1–C3), and higher At% of C and Cl (~20.0 and ~35.6%, Figures 6B1–C3).

EDS analysis of enamel in wild-type and double-mutant mandibular incisors. WT, Wild-type; DM, Double-mutant; At%, Atomic percentage. (A1,A2) EDS spectrum of enamel at the first reference plane. (A3) Between wild-type and double-mutant enamel at the first reference plane, there were no statistically significant differences in the atomic percentages (At%) of all the elements analyzed—Ca, P, O, C, Cl, Na, and Mg. (B1,B2) EDS spectrum of enamel at the second reference plane. (B3) Statistically significant changes were detected in the At% of Ca, P, C, and Cl. The At% of Ca and P in double-mutant enamel decreased by ~26.7 and ~35.1%, respectively, compared to those in wild-type enamel. There were increases in the At% of C and Cl— ~268.4 and ~18.6%, respectively (double-mutant/wild-type). (C1,C2) EDS spectrum of enamel at the third reference plane. (C3) Double-mutant enamel showed significantly lower At% of Ca, P, O, Mg (~92.8, ~69.2, ~29.6, and ~57.9%), and higher At% of C and Cl (~20.0 and ~35.6%).

 Deletion of <italic>Slc26a1</italic> and <italic>Slc26a7</italic> does not affect morphology of ameloblasts

We prepared tissue sections from 4-week-old mouse mandibles (wild-type and double-mutant) for H & E staining. At the regions marked by the three reference planes, wild-type enamel organs demonstrated typical morphology of ameloblasts in late-maturation, maturation, and secretory stages (Figures 7A1–A3). Compared with the findings in the wild-type group, cell morphology in double-mutant enamel organs in the same regions was not significantly different (Figures 7B1–B3).

Histological analysis of wild-type and double-mutant enamel organs by H& E staining. WT, Wild-type; DM, Double-mutant; ES, Enamel space; Am, Ameloblast; PL, Papillary layer; CT, Connective tissue; SI, Stratum intermedium; SR, Stellate reticulum. (A1–A3) Wild-type enamel organ in late-maturation, maturation and secretory stages (labeled by three reference planes 1, 2, and 3). (B1–B3) Double-mutant enamel organ at the three reference planes. Magnification 40x. Compared to the wild-type group, cell morphology in double-mutant enamel organs in the same regions was not significantly different.

 pH regulators show compensatory expression in double-mutant animals

The expression levels of 16 genes involved in pH regulation and ion transport during maturation-stage amelogenesis were quantified by realtime PCR using RNA samples isolated from wild-type and double-mutant maturation-stage enamel organs. Significant upregulation was detected for all the genes quantified (double-mutant/wild-type, Figure 8). Note that Ae4 and Slc26a9 showed the most striking fold changes—~70.5 and ~83.0%, respectively (Figure 8B), and the fold changes for the remaining genes were all above 2, except for Lamp3, Rab21, and Nhe1 (Figure 8B).

Realtime PCR analysis of gene expression in wild-type and double-mutant maturation enamel organs. WT, Wild-type; DM, Double-mutant. (A) Relative expression values normalized to that of Beta-Actin. (B) Fold changes. Significant upregulation was detected for all the genes quantified (DM/WT). Ae4 and Slc26a9 showed most striking fold changes—~70.5 and ~83.0%, respectively. The fold changes for the remaining genes were all above 2, except for Lamp3, Rab21, and Nhe1. *P < 0.05; **P < 0.01.

 Discussion

Enamel formation during maturation-stage amelogenesis involves mineral deposition, crystal growth, protease activities and the degradation of the internalized organic matrix, all of which are highly pH-dependent (Simmer and Fincham, 1995; Smith et al., 1996; Smith and Nanci, 1996; Lacruz et al., 2010a, 2012b). Acid-base balance in the extracellular matrix and intracellular lumens is maintained by a complex regulatory network involving multiple ion transporters and carbonic anhydrases (Dogterom and Bronckers, 1983; Lin et al., 1994; Wright et al., 1996a,b; Arquitt et al., 2002; Lyaruu et al., 2008; Paine et al., 2008; Bronckers et al., 2009, 2010; Josephsen et al., 2010; Wang et al., 2010; Lacruz et al., 2010a,b, 2012c, 2013a; Chang et al., 2011; Duan et al., 2011; Duan, 2014; Jalali et al., 2014; Reibring et al., 2014; Wen et al., 2014). Although details regarding the mechanism of pH control are yet to be clarified, the critical roles of many genes in maturation-stage pH regulation have been implicated by previous studies on transgenic animal models. For example, NBCe1 is a sodium-bicarbonate cotransporter expressed mainly on the basolateral membrane of maturation-stage ameloblasts (Lacruz et al., 2010b; Jalali et al., 2014). NBCe1−/− animals demonstrated hypomineralized and weak enamel with an abnormal prismatic architecture. Severe enamel phenotypes have also been documented from Cftr−/− and Ae2−/− animals (Arquitt et al., 2002; Lyaruu et al., 2008; Bronckers et al., 2010; Chang et al., 2011). Bronckers et al. started to investigate the role of Slc26 family genes in tooth enamel formation in 2011 (Bronckers et al., 2011). Since then, all the animal studies on Slc26 mutations have reach similar conclusions: mutation or silencing of individual Slc26 gene members (Slc26a1, Slc26a3, Slc26a4, Slc26a6, and Slc26a7) is not sufficient to generate abnormal enamel phenotypes, yet the deletion of a single Slc26 gene can induce strong compensatory expression of other pH regulatory genes and SLC26 family members (Bronckers et al., 2011; Jalali et al., 2015; Yin et al., 2015).

In the present study, we continued with our previous investigation of Slc26a1−/− and Slc26a7−/− animal models. We generated a double-null animal line with the absence of both Slc26a1 and Slc26a7 (Slc26a1−/−/Slc26a7−/−). The enamel density of double-null animals was significantly lower in the regions that represent late maturation-, maturation- and secretory-stage enamel development in age-matched wild-type siblings (Figures 2, 3). However, the difference in enamel density between double-mutant and wild-type mandibular first molars was not statistically significant, which suggests that incisor and molar maturation events differ to some extent (Figure 4). In addition, the “maturation” and “secretory” enamel microstructures in double-mutant animals resembled those observed in wild-type secretory and/or pre-secretory stages (Figure 5). This indicates that deletion of Slc26a1 and Slc26a7 delayed enamel development in mandibular incisors, although such an impact was not observed after full eruption of the mandibular first molars in double-mutant animals (only data from 4-week-old animals are shown in Figure 4). Subsequent elemental composition analysis of double-mutant incisors revealed that decreased enamel density could be attributed to a lack of mineral deposition (Ca2+ and HPO3, Figure 6). The accumulation of Cl− in double-mutant enamel was consistent with our previous findings in Slc26a1−/− and Slc26a7−/− animals (Yin et al., 2015), while the increase of carbon in double-mutant enamel is a possible manifestation of disrupted EMP retrieval and hydrolysis (Figure 6). These findings indicate functional redundancy within the SLC26 gene family, and also in the scope of the pH regulatory network during enamel maturation (Yin et al., 2015). Such a redundancy is not uncommon in developmental processes and pathogenesis of diseases, e.g., matrix metalloproteinases (MMPs) in embryonic development and amyloid precursor protein (APP) genes in Alzheimer‘s disease (Heber et al., 2000; Page-McCaw et al., 2007).

Amelogenesis imperfecta (AI) is the most severe inherited disorder among all enamel pathologies. The genes responsible for AI in human patients include AMELX, AMBN, ENAM, MMP20, KLK4, WDR72, FAM83H, LAMB3, ITGB6, and SLC24A4, and current evidence tends to support a single-gene origin for many AI cases (Aldred et al., 1992; Lench et al., 1994; Lagerstrom-Fermer and Landegren, 1995; Lagerstrom-Fermer et al., 1995; Collier et al., 1997; MacDougall et al., 1997; Hart et al., 2000, 2003, 2004, 2009; Kindelan et al., 2000; Mardh et al., 2002; Kim et al., 2004, 2005, 2008, 2013; El-Sayed et al., 2009; Wright et al., 2009; Poulter et al., 2014a,b,c; Wang S. et al., 2014; Wang S. K. et al., 2014; Herzog et al., 2015). Our data from the double-mutant animals (Slc26a1−/−/Slc26a7−/−) suggest that polygenic etiologic factors might also be involved in the pathogenesis of AI/AI-like symptoms, which increases the complexity of genetic diagnosis for enamel disorders. The statement is further corroborated by the findings from a recent study on BMPs, in which double deletion of Bmp2 and Bmp4 in the epithelium led to hypoplastic enamel in mice (Xie et al., 2016).

We proposed in our previous study that pH regulation during enamel maturation might be achieved by the coordination of functional protein complexes (Yin et al., 2015). This is based on our findings that physical protein-protein interactions exist between Cftr and Slc26 gene family members Slc26a1, Slc26a6, and Slc26a7 in maturation-stage ameloblasts, as supported by colocalization analyses, including co-immunofluorescence and co-immunoprecipitation studies. Here we examined the co-distribution pattern of SLC26A1 and SLC26A7 in maturation-stage ameloblasts by conducting immunostaining. We did not observe any overlaps in fluorescence of SLC26A1 and SLC26A7, which indicates a possible lack of colocalization of these two anion exchangers on the apical membrane of ameloblasts (Figure 1A). Nevertheless, the interactions between other different pH regulators in enamel maturation still warrants further investigation.

In conclusion, the data obtained from Slc26a1−/−/Slc26a7−/− mutant mice provide new evidence in support of the hypothesis that SLC26A1 and SLC26A7 are actively involved in the ameloblast-mediated pH regulation process during maturation-stage amelogenesis.

 Author contributions

KY, JG, MS and MP designed the experiments; KY and WL performed the experiments; MS developed the mutant animal model; KY, JG, SR and MP analyzed the data; KY and JG prepared the Figures and tables; and KY and MP wrote the manuscript. All listed authors critically read, edited, and approved the final manuscript. MP accepts full responsibility for the integrity of the data analysis.

 Funding

This work was supported by NIH/NIDCR [grants # R01 DE019629 and R21 DE024704 (MP), R90 DE021982 (KY), and from the Department of Veterans Affairs [grant - Merit Review 5 I01 BX001000-06 award (MS)].

Conflict of interest statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

We sincerely thank Thach-Vu Ho and Dr. Jingtan Su (University of Southern California) for their assistance in μCT scanning and EDS analysis. We also thank Bridget Samuels for her critical reading and editing of the manuscript.

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