Department of Oral Biochemistry, Institute of Odontology, Sahlgrenska Academy, University of Gothenburg, Göteborg, Sweden.
Address correspondence to: Amel Gritli-Linde, Department of Oral Biochemistry, Sahlgrenska Academy, University of Gothenburg, Medicinaregatan 12F, SE–41390 Göteborg, Sweden. Phone: 46.31.786.3386; Fax: 46.31.418122; E-mail: email@example.com.
First published April 26, 2010 - More info
Cleft lip and cleft palate, which can also occur together as cleft lip and palate, are frequent and debilitating congenital malformations, with complex geneses that have both genetic and environmental factors implicated. Mutations in the genes encoding the p53 homolog p63 and interferon regulatory factor 6 (IRF6) are major causes of cleft lip and cleft palate, but the molecular and cellular mechanisms underlying this have not been clear. However, in this issue of the JCI, Thomason et al. and Moretti et al. independently show that p63 and IRF6 operate within a regulatory loop to coordinate epithelial proliferation and differentiation during normal palate development. Disruption of this loop as a result of mutations in p63 or IRF6 causes congenital clefting.
The developing organism is a master at using simple paradigms to generate complexity. This is typified by the use, at least during early organogenesis, of the same molecular pathways to drive the development of organs and tissues as diverse as the brain, limbs, teeth, and skin. This, however, has a major disadvantage, in that disruption of a specific molecular pathway can lead to concomitant dysfunction of multiple organs, a condition clinically classified as a syndrome.
In humans, mutations in the gene encoding the transcription factor p63, a p53 homolog, cause several autosomal dominant ectodermal dysplasia syndromes (i.e., syndromes deriving from abnormalities in ectodermal structures, such as the hair, teeth, nails, sweat glands, craniofacial structures, and digits), including ectrodactyly-ectodermal dysplasia-clefting (EEC) and ankyloblepharon-ectodermal dysplasia-clefting (AEC) syndromes. These are both characterized by cleft lip and/or cleft palate (CL/CP) and defects in ectoderm-derived tissues, such as the epidermis, hair, teeth, and glands (1). Clinically, AEC syndrome differs from EEC syndrome by the near absence of digit malformations and the occurrence of eyelid fusions (ankyloblepharon) and severe skin erosions (1). Similarly, mutations in the gene encoding the transcription factor interferon regulatory factor 6 (IRF6) cause van der Woude syndrome (VWS) and popliteal pterygium syndrome (PPS), both of which are characterized by many ectodermal anomalies, including CL/CP (2). p63 and IRF6 mutations also have been implicated in nonsyndromic forms of CL/CP (i.e., forms of CL/CP in which the lip and/or palate are the only affected tissues) (3).
A first glimpse of the physiological roles of p63 and IRF6 came from studies of mutant mice. p63-null mice lack a stratified epidermis, teeth, hair, and several exocrine glands and display limb truncations as well as CL and CP (4, 5). The skin defects are caused by impaired proliferation and differentiation of epidermal keratinocytes (4). Mice either null for Irf6 (6) or homozygous for R84C (7), a common IRF6 mutation in individuals with PPS, replicate several anomalies found in patients with VWS and PPS, including skin impairment and the aberrant intraoral epithelial adhesions that lead to CP. The abnormal development of the skin is due to the inability of epidermal keratinocytes to stop proliferating and to undergo terminal differentiation (6, 7).
The discovery that mutations in the genes encoding p63 and IRF6 cause human ectodermal dysplasia syndromes triggered a chain reaction of research aimed at unravelling their functions and identifying their targets during normal and abnormal epithelial development (4–8). Yet, their mode of action, regulation, and targets during normal lip and palate development and the mechanisms behind the genesis of CL/CP in both humans and mouse models are still largely unknown. However, in this issue of the JCI, Moretti et al. (9) and Thomason et al. (10) identify an intriguing relationship between p63 and IRF6 during palate development (well illustrated in Figure 5 in ref. 9) by using an arsenal of experimental strategies.
Studies of the functions of p63 are complicated by the existence of at least six different isoforms. Two separate transcription start sites generate the ΔNp63 isoforms and the p53-like TAp63 isoforms. Transcripts of both the TAp63 and ΔNp63 isoforms undergo alternative splicing, generating three subtypes each, designated α, β, and γ (4). Here, the term p63 is adopted to refer to experiments and data that do not distinguish between the TAp63 and ΔNp63 isoforms, while ΔNp63 is used to describe experiments and findings that do not distinguish between the α, β, and γ subtypes of this isoform.
In the search for putative targets of p63, Moretti et al. (9) identified Irf6 as a positively regulated target of ΔNp63. Given that IRF6 and p63 are expressed in stratified epithelia, and because of the similarities between the organs affected in humans and mice with mutations in the genes encoding IRF6 and p63, Thomason and coworkers (10) hypothesized that these transcription factors may in fact interact. They generated compound heterozygotes for p63 and Irf6R84C (p63+/–Irf6+/R84C mice) and found that, in contrast to the single heterozygotes, which were devoid of CP, the double heterozygotes exhibited a fully penetrant CP, indicating a genetic interaction between Irf6 and p63.
Expression analyses using palates and epidermis from mice with mutations in p63 and keratinocytes and epidermis from patients with EEC and AEC syndromes, combined with in vitro mutagenesis, demonstrated that expression of IRF6 requires normal function of ΔNp63 (9, 10). Using in vitro genetic manipulation and biochemical assays, the authors show that IRF6 is directly activated by ΔNp63α (9, 10) but not by TAp63 (9). Importantly, disease-causing mutations in p63 abrogated the ability of p63 to activate IRF6 transcription in vivo and in vitro (9, 10).
These findings are clinically important, as they suggest that IRF6 can acts as a modifier gene to affect p63 disease outcomes and that polymorphisms in the newly identified p63-binding site, in an upstream enhancer element of IRF6 (10), may be involved in the subset of individuals with VWS and PPS, in which the causative IRF6 mutations have remained elusive, as well as in some forms of nonsyndromic orofacial clefting. As the p63-binding site upstream of the IRF6 gene was found to overlap with a recently identified enhancer element of IRF6, in which a single nucleotide polymorphism associated with cleft lip disrupts binding of the transcription factor AP-2α (11), Thomason et al. (10) suggest it is likely that p63 and AP-2α co-operate in the regulation of IRF6.
The sequences of secondary palate development (i.e., development of the structure that separates the nasal cavity from the oral cavity, allowing simultaneous breathing and eating) in humans and mice are similar and tightly regulated by epithelial-mesenchymal interactions (3). Initially, the bilateral palatal shelves (PSs), which are composed of a core of mesenchyme covered by an epithelium, grow downward from the maxillary primordium (Figure 1A). Subsequently, the PSs elevate into a horizontal position (Figure 1B) and contact each other through their medial edge epithelia (MEE), which, after adhesion, form a transient medial epithelial seam (MES) made of nonproliferating cells (Figure 1, C and D). The periderm, a layer of flat cells that cover external epithelia in embryos, is required for establishing the first firm contact of MEE through filopodia (polarized cell protrusions). Adhesion of the opposing MEE occurs by junctional complex proteins (Figure 1E). Thereafter, apoptosis seals the fate of the MES (Figure 1F). The quick degeneration of the MES allows mesenchymal continuity and successful palate closure (Figure 1G). Similarly, upper lip and primary palate development proceed by growth, morphogenesis, and fusion of facial primordia (3). The primary palate forms the anterior-most structure of the upper jaw, the premaxilla, from which the four upper incisor teeth arise. Disruption of these steps results in CL/CP (Figure 1H). These sequences may seem simple; however, each stage of lip and palate development is governed by an impressive number of molecular pathways (3).
Development of the mouse secondary palate and human CL/CP. (A–G) Histological sections of mouse embryo heads, showing the development sequences of the secondary palate. (A) At E14, the PSs are vertically oriented in the oral cavity. (B) At E14.5, the PSs have elevated to a horizontal position above the dorsum of the tongue (T). (C and D) At E15, adhesion of the PSs, through their MEE, creates the MES. (D) A high-magnification image of the PS shown in C. (E) Immunohistochemistry showing expression of zonula occludens 1, a tight junction component (dark color), in the regressing MES and the rest of the palate epithelium. (F) Immunostaining for cleaved lamin A, showing apoptotic cells (dark spots indicated by arrows) in the MES and in the epithelial seam at the nasopalatine junction (NPJ), the site of adhesion between the PS and the nasal septum. (G) Successful closure of the palate (P) at E15.5 leads to the separation of the oral and the nasal cavities (NC). (H) Infant with unilateral total clefts of the lip, alveolar ridge, primary palate, and secondary palate. Asterisks indicate tooth primordia. Scale bars: 500 μm (A–C and G); 100 μm (D and F); and 50 μm (E).
Although the palatal MEE of p63+/–Irf6+/R84C compound heterozygote embryos were able to abut, they ignored each other, adhesion failed, and the palate remained cleft (10). In these mutants, an abnormal differentiation of the MEE and failure of polarization of peridermal cells prevented adhesion of the PS. In Irf6R84C/R84C embryos, the MEE fails to disintegrate at sites of ectopic adhesion, suggesting a defective epithelial differentiation (12).
In mice, abrogation of TGF-β signaling in the MEE leads to a complete loss of Irf6 expression (3), suggesting that Irf6 functions downstream of TGF-β during palatal fusion. Normal TGF-β activity is an absolute requirement for MES disintegration by apoptosis, a prerequisite for fusion. Remarkably, loss of signaling via the type II TGF-β receptor leads to CP, as a result of unchecked proliferation of MES cells that fail to die (3, 13), a situation that seems to result from failure of induction of the TGF-β target gene p21, which encodes a cyclin-dependent kinase inhibitor (13). Interestingly, ΔNp63α has been shown to directly repress transcription of p21 and the stratifin gene (Sfn) encoding another antiproliferative cell cycle mediator, and this activity is strongly diminished in cells expressing mutant forms of ΔNp63α (14). In mice, Sfn and Irf6 have been found to interact genetically (7).
All these observations point to intricate interactions between TGF-β signaling, IRF6, and p63 during palatogenesis. TGF-β signaling exerts roles in tumor suppression and metastasis, and recent findings point to a tumor suppressor function for p63, which promotes the oncogenic function of TGF-β in cancer cells when it is lost subsequent to its TGF-β–dependent sequestration by mutant p53 (15). IRF6 mRNA and protein are totally lost in metastatic breast cancer cell lines and in invasive breast ductal carcinomas (8). These observations suggest that TGF-β, p63, and IRF6 also interact in cancer.
Inasmuch as p21 expression is required for MES disintegration (13), and because ΔNp63α represses p21 expression (14), one would imagine that for p21 to be expressed in the MES, p63 must disappear. Indeed, Thomason et al. (10) found that in WT embryos, upon formation of the MES following adhesion of the MEE, p63 protein was spirited away, whereas Irf6 reached the pinnacle of its expression. Intriguingly, the MEE of Irf6R84C/R84C mutants remained p63 positive, indicating that p63 downregulation necessitates normal IRF6 function (10). Similarly, Moretti et al. (9) found a reciprocal relationship between IRF6 and p63 proteins, both in human skin sections and in differentiating keratinocytes, leading the authors to posit that following transcriptional activation of IRF6 by ΔNp63, IRF6 promotes the decay of ΔNp63, allowing keratinocytes to exit the cell cycle and differentiate. This hypothesis was validated by experimental assays showing that differentiation-induced decrease of ΔNp63 protein levels and terminal differentiation of keratinocytes required IRF6 activity (9).
What happens to p63? Its fate turns out to be proteasomal degradation. While this finding concurs with those of previous studies, indicating proteasomal degradation of WT but not mutant ΔNp63 (16–18), the treasure that was unearthed by Moretti et al. (9) was that IRF6 itself targets the ΔNp63α and ΔNp63β isoforms to proteasomal degradation. Moreover, they show that a mutant ΔNp63 protein corresponding to one that causes EEC syndrome is resistant to IRF6-mediated downregulation, whereas the product of IRF6R84C is unable to induce ΔNp63 protein downregulation. These elegant studies provide a clear explanation as to the perdurance of ΔNp63 protein in the MEE of Irf6R84C/R84C mutant mice (10). Thus, WT IRF6 turns against its inducer; however, this treacherous act is intended for a good cause: preventing orofacial clefting and other ectodermal anomalies.
Together, the studies by Moretti et al. (9) and Thomason et al. (10) demonstrate that IRF6 and p63 function in a biological regulatory loop to coordinate epithelial proliferation and differentiation. Furthermore, they show that disease-causing mutations in IRF6 or p63 interrupt this loop and lead to disruption in epithelial development and subsequently to severe malformations, including CL/CP.
While the findings of Moretti et al. (9) and Thomason et al. (10), together with the initial study of the mechanisms leading to CL in p63–/– embryos (5), enhance our understanding of the molecular and cellular events controlled by IRF6 and p63 during normal and abnormal development of the lip and palate, they clearly set the stage for human genetic studies to define the etiology of nonsyndromic forms of orofacial clefting. Recent advances (19) provide hope that direct targets of IRF6 can be identified and then assessed as potential causal genes in orofacial clefting. Since p63 and IRF6 are known to be involved in cancer (1, 8, 15) and in view of the present findings (9, 10), it wouldn’t be surprising if the p63-IRF6 relationship were disrupted in cancer, albeit with variation inherent to neoplasia.
Naturally, the findings of Moretti et al. (9) and Thomason et al. (10) generate questions. How does IRF6 promote ΔNp63α proteasomal degradation? At least in cancer cells, stratifin seems to indirectly target phosphorylated ΔNp63α to the proteasome by escorting it out of the nucleus, while the proteasomal targeting itself is executed by RACK1, which has been suggested to function as an E3 ubiquitin ligase (20). However, there are precedents for SUMO1- and ubiquitin-mediated proteasomal degradation of ΔNp63α (16–18). Is IRF6 engaged in direct or indirect induction of some key factor(s) in the sumoylation or ubiquitylation cascades? For example, SUMO1 itself or a specific ubiquitin ligase could be potential targets. Of note, several key players in lip and palate development have been shown to be substrates for sumoylation by SUMO1, and altered function of SUMO1 in humans and mice results in orofacial clefting (3). Compound heterozygous Sumo1+/–p63+/– mice may prove informative in this regard. IRF6 is also a substrate for proteasomal degradation, following phosphorylation and ubiquitination (8); however, the molecular mechanisms behind its posttranslational modification are still unknown. How does the IRF6-p63 regulatory loop integrate into other signaling pathways under normal and diseased states?
Collaboration between clinicians, geneticists, and basic scientists as well as the clever use of mouse models will certainly help address some of these questions and enhance our understanding of IRF6- and p63-related diseases, the ultimate beneficiaries being the afflicted patients and their families.
I am grateful to Anders Linde for preparing the figures and to Sara Rizell for providing the clinical photo. The author is supported by the Swedish Research Council-Medicine (grants 15181 and 20614), the Institute of Odontology at Sahlgrenska Academy, and the Thuréus Foundation.
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