Search tips
Search criteria 


Logo of jbbJournal's HomeManuscript SubmissionAims and ScopeAuthor GuidelinesEditorial BoardHome
J Biomed Biotechnol. 2011; 2011: 864904.
Published online 2011 May 22. doi:  10.1155/2011/864904
PMCID: PMC3118300

A Symphony of Regulations Centered on p63 to Control Development of Ectoderm-Derived Structures


The p53-related transcription factor p63 is critically important for basic cellular functions during development of the ectoderm and derived structure and tissues, including skin, limb, palate, and hair. On the one side, p63 is required to sustain the proliferation of keratinocyte progenitors, while on the other side it is required for cell stratification, commitment to differentiate, cell adhesion, and epithelial-mesenchymal signaling. Molecules that are components or regulators of the p63 pathway(s) are rapidly being identified, and it comes with no surprise that alterations in the p63 pathway lead to congenital conditions in which the skin and other ectoderm-derived structures are affected. In this paper, we summarize the current knowledge of the molecular and cellular regulations centered on p63, derived from the comprehension of p63-linked human diseases and the corresponding animal models, as well as from cellular models and high-throughput molecular approaches. We point out common themes and features, that allow to speculate on the possible role of p63 downstream events and their potential exploitation in future attempts to correct the congenital defect in preclinical studies.

1. The p63 Gene: Structure and Function

The TP63 gene codes a transcription factor homologous to the p53 tumour suppressor protein and is translated into six protein isoforms: the TransActivating (TA) isoforms are more closely resembling p53, while the Delta-N (ΔN) isoforms are devoid of the TransActivation (TA) domain 1 (TA1). Although the TA isoforms were initially thought to be the only ones to possess transcriptional regulatory functions, it has been well established that the ΔN isoforms are also able to activate transcription of a distinct set of target genes via a second TA domain (TA2) [1]. Initially, TA and ΔN isoforms with three alternative carboxyl termini (α, β, and γ), generated by alternative splicing, were identified. However, like for p73, additional p63 isoforms (δ and ε) have been recently described [2].

The p63 protein contains a TA domain, a DNA-Binding Domain (DBD) and an Oligomerization Domain (OD). Both the TA and [increment]N alpha-isoforms also contain a Sterile Alpha Motif (SAM) domain, which is absent in p53 [3]. SAM domains are protein-protein interaction modules found in developmentally relevant proteins [4]. Recent studies have identified a Transcriptional Inhibitory (TI) domain located between the SAM domain and the C-terminus of p63α; this domain is believed to be responsible for the lower transactivation ability of TAp63α compared to the -β and the -γ  isoforms [5].

p63 is highly conserved among a wide range of organisms. Interestingly, in the genome of Danio rerio (zebrafish) the mammalian type TA coding sequence is missing; therefore, only the ΔN isoforms are present [6]. Both mice and zebrafishes lacking p63 expression fail to develop a normal epidermis and show malformations of appendages and other structures that require epithelial-mesenchymal interactions during development [79].

2. Human Diseases Linked to p63

The p63 locus is consistently transcribed by basal stem cells of stratified epithelia, by myoepithelial cells of the breast and salivary glands, and by the proliferative compartment of the gastric mucosa [10, 11]. The expression of the ΔNp63 and TAp63 classes of isoforms is quite distinct and changes dynamically during development and maturation of the ectoderm (towards the epidermis) and derived structures (hair follicles, limbs, glands) [11, 12]. Unlike p53, p63 does not act as a classical tumour-suppressor, although its involvement in tumor progression is being increasingly recognized [13, 14]. p63 plays a prominent role in the control of epithelial stem cell functions and in the differentiation and stratification of ectoderm-derived tissue during embryonic development.

A wide spectrum of autosomal-dominant hereditary diseases is associated to mutations of the p63 gene, in humans. A common feature of these disorders is the appearance of Ectodermal Dysplasia (ED), a phenotypic group that comprises abnormal maturation and stratification of the skin and abnormal development of hairs, teeth, nails, esocrine glands, and cornea. The other two consistent features of p63-linked disorders are Cleft Lip/Palate (CL/P) and ectrodactyly, also known as Split Hand/Foot Malformation (SHFM). Ectrodactyly is a limb developmental malformation characterized by a medial cleft, missing central digits and often fusion of the remaining ones [15].

Human autosomal dominant syndromes associated with heterozygous p63 mutations are Ectrodactyly-Ectodermal dysplasia-Cleft lip/palate syndrome (EEC, MIM 106260), Limb-Mammary Syndrome (LMS, MIM 603543), Ankyloblepharon Ectodermal dysplasia Clefting (AEC, MIM 106260), and nonsyndromic Split-Hand/split-Foot Malformation-type IV (SHFM-IV) (MIM 605299) [1620]. EEC is the most prominent congenital disorder and is characterized by the three phenotypes: ED, ectrodactyly, and CL/P. EEC is almost invariably caused by heterozygous mutations in the DBD of p63 [21, 22]. Nonetheless, p63 mutations can explain only a minority of patients with isolated or nonsyndromic ectrodactyly (about 10%) or cleft lip/palate (about 0.1%).

In addition to SHFM-IV, associated to p63 mutations, ectrodactyly appears as an isolated nonsyndromic disorder linked to mutations or chromosomal anomalies in distinct loci [20, 23, 24]. Of these, gene mutations have been identified only for SHFM-VI (MIM 225300, the only autosomal recessive form) and for Ectodermal Dysplasia-Ectrodactyly-Macular Dystrophy syndrome (EEM, MIM 225280). In SHFM-VI, homozygous mutations of the WNT10B gene have been found [25]. In EEM patients, mutations in the P-cadherin (or cadherin-3, or CDH3) gene have been found [26, 27]; this gene codes for an adhesion molecule of the cadherin class, expressed by the AER cells of the embryonic limb buds. However, the targeted deletion of P-cadherin in mice does not cause limb defects [28]. It is not known, at the moment, if a regulatory link exists between p63 and these two SHFM disease genes.

SHFM-I (MIM 183600) is linked to deletions, inversions, and rearrangements affecting chromosome 7q21 [2931]. The smallest region of overlapping deletions encompasses several genes: DYNC1l1, SLC25A13, DSS1, DLX5, and DLX6; of these only DLX5 and DLX6 have been shown to be specifically expressed in the AER of the developing limb buds [3234]. Importantly, the murine models of Dlx5;Dlx6 inactivation establish that their misregulation is etiological to SHFM-I [33, 34], and Dlx5 and Dlx6 are now recognized as transcriptional targets of p63 [35, 36].

SHFM-III (MIM 600095) is associated with complex duplications/rearrangements around the DACTYLIN (FBXW4) gene, on chromosome 10q [37]. The genomic lesion involves the DACTYLIN, LBX1, and  βTRCP genes, but none of these genes is directly disrupted and no point mutation has been reported. Interestingly, FGF8 and NFkB2, two genes implicated in limb development, are located in the proximity of the rearrangement breakpoints [3841].

Finally, SHFM-V (MIM 606708) is associated to deletions encompassing the HOXD gene cluster, near DLX1 and DLX2 [4244]. The X-linked SHFM-II form (MIM 313350) has been mapped to chromosome Xq26.3 [45], but no disease gene has yet been identified.

Diseases grouped within the same phenotypic class are likely to be caused by genetic abnormalities or misregulation of functionally related genes, or genes that are component of a regulatory network [4648]. Elucidation of functional interactions among genes within the p63 network, their encoded proteins, and regulatory elements controlling their expression is bound to provide new candidate genes for genetic disorders linked to p63.

3. Genotype-Phenotype Correlations

In the EEC spectrum syndromes, the position and type of p63 mutation (frameshift, missense, deletion) correlate with the observed phenotype. p63 mutations causing EEC are usually not found in AEC, LMS, and SHFM [1619]. The vast majority of EEC mutations are missense mutations in the DBD, generating aminoacid substitutions in the residues predicted to contact DNA. In these cases, all p63 isoforms are affected by these mutations. DBD mutants usually act as dominant-negative effectors and render the WT protein unable to bind DNA [21], explaining the dominant transmission of EEC. Mutations in exons 13 and 14, affecting only the α isoform of p63, have been found associated to all four syndromes.

SHFM-IV results from mutations either in the DBD or in the C-terminal domain of p63α, whereas the AEC syndrome is exclusively associated with heterozygous missense mutations in the SAM domain. The α tail of p63 contains a sumoylation site, inactivated by p63 mutations found in SHFM-IV (E639X). Sumoylation can modulate p63 half-life [1], and naturally occurring mutated p63 proteins often display altered stability, suggesting that the final effect of the mutations could be the persistence of the mutated protein and consequent misexpression of p63 targets.

Finally, for a large set of disorders with features of ED and resembling p63-caused syndromes (referred to as p63-linked phenotype spectrum), the molecular lesion is unknown [49].

Attempts to unequivocally establish the role of p63 in human ectodermal syndromes are hampered by the fact that this protein exists in multiple isoforms with different, often contradictory, biological activities; moreover, some of the mutations are isoform-specific (affecting only the α isoform) while others affect all isoforms.

Therefore, the mode of action of p63 mutations (haploinsufficiency? dominant-negative?) is still debated. For the same reason, the possibility to use wild-type p63 for pharmacological purposes or for gene delivery appears unrealistic.

4. Animal Models of p63-Linked Diseases

Much of our current knowledge on the role of disease genes for ectoderm development and limb morphogenesis has been gathered via the generation of animal models of the EEC, AEC, and SHFM, and the analysis of their phenotypes at cellular and developmental level. Mice null for p63 have been generated by two groups independently [50, 51]; at birth these mice show severe defects affecting their skin, limb and craniofacial skeleton, teeth, hair, and mammary glands. Specifically, the skin appears thin, mostly single-layered and translucent, unable to prevent water loss. The hindlimbs (HL) fail to form altogether, while the forelimbs (FL) are severely truncated and lack most of their distal skeletal elements. The altered phenotypes observed in these mutant mice are a direct consequence of altered cellular properties affecting the same tissues and organs as in human EEC, thus these mice have been considered as models of human EEC [21, 5052].

However, there are some caveats intrinsic to the p63 null mice as model of EEC. First, in the p63 null model named Brdm2 [50], gene inactivation was achieved by insertional mutagenesis, which however resulted in a partial gene duplication. Although the p63 protein is undetectable in these mice, their skin shows patches of stratified epithelium that appear to reexpress p63, and it is currently unclear whether these are due to aberrant transcription of the mutated p63 gene or represent spontaneous phenotypic reversal [53]. Second, and this is the major concern, loss of p63 in the germline is not synonymous of the presence of one mutated allele, the situation commonly observed in EEC patients. While in the null animals the p63 protein is missing altogether (i.e., both the TA and ΔN isoforms), in EEC, AEC, LMS, and SHFM-IV patients the mutated p63 protein coexists with half of the normal dose of wild-type p63. Hence, the p63 null mice might not accurately recapitulate the molecular pathogenesis of these syndromes.

To circumvent this problem, the group of Dr. A. Mills (CSHL, USA) has generated a new line of mice bearing the R279H mutation in p63 (a mutation found in EEC patients) in their germline. Homozygous embryos and newborn animals show a global phenotype similar, but not identical, to that of p63 null animals [35], consisting in the absence of the HL, severely truncated FL, a thin translucent skin and craniofacial and palatal defects. The HL defects in both the p63 null- and the p63-R279H homozygous embryos are evident as early as E9.5, accompanied with loss of AER stratification [35, 50, 51]. Interestingly, heterozygous p63-R279H mutant embryos and newborns show a poorly penetrant EEC phenotype characterized by mild skin hyperplasia, cleft palate, and ectrodactyly. In particular, the skin of these animals shows patches of hyperplasia, in which Irf6 and IKKα expression is markedly reduced, while p63 nuclear expression is increased. The same can be observed in skin of AEC patients [54, 55]. Thus, the p63-R279H heterozygous mice display a global phenotype that resembles human EEC more closely than the phenotype of p63 null mice.

Mice have been generated in which ΔNp63 is downregulated in the developing epidermis, as a model for AEC [56]. In fact, the AEC-mutated variants of ΔNp63 have been shown to exert a dominant-negative action on the wild-type protein. Reduced ΔNp63 expression in the mouse epidermis causes severe skin erosion consequent to suprabasal cell proliferation, retarded terminal differentiation and basement membrane abnormalities [56], a condition that closely resembles the AEC phenotype.

Mouse models for SHFM-I have been generated by the combined deletion of Dlx5 and Dlx6 [33, 34]; in these animals ectrodactyly is observed at the HL, the AER is induced normally, however, by E10.5 the expression of FGF8 and other markers declines in the central sector of the limb bud, accompanied with a loss of stratification in the same region [31, 32] (G.M. and LoIacono, unpublished).

The Dactylaplasia (Dac) mutant mouse strain has been proposed as a model of SHFM-III [57, 58]. The AER of Dac heterozygous embryos shows reduced FGF8 expression and defective cell layering [59]. However, the role of Dactylin as the disease gene in SHFM-III is currently doubted, since the rearrangements/duplications around the Dactylin locus do not disrupt or interrupt the gene, and since Dactylin is ubiquitously expressed in mouse tissues.

Finally, zebrafish p63 morphants have been reported [6, 60]. Interestingly, they share some phenotypic features with human EEC patients and might be used for developmental studies. In this model, ΔNp63 expression is tightly regulated by Smad4/5-mediated Bone Morphogenetic Proteins (BMP) signaling, and it acts as a transcriptional repressor that blocks anterior neural specification and conversely promotes early steps of epidermal specification. Forced expression of ΔNp63γ blocks neural development even in the absence of BMP signal [6]. We should point out, however, that the skin and fins of fishes are not fully comparable to the mammalian limbs [61], and therefore the information gained from the fish model might not fully translate to the mammalian system.

5. The Role of p63 for Keratinocyte Proliferation and Differentiation

The best experimentally characterized function of p63 is to maintain the proliferative potential of epidermal progenitor cells [62, 63]. In addition to this, p63 also impacts on epidermal stratification and keratinocyte differentiation. Specifically, ΔNp63 is required for the initial commitment of keratinocyte progenitors towards differentiation [10, 62], although for differentiation to proceed ΔNp63 needs to be subsequently eliminated [64, 65]. The depletion of ΔNp63 occurs mainly via proteasome-mediated degradation [6668], which in turn is controlled by several proteins some of which are transcriptional targets of ΔNp63 [55, 69, 70]. In addition, the expression of a p63-specific microRNA (miR203) is also important to induce p63 downregulation during terminal differentiation [71].

p63 regulates transcription via binding to p63-Response Elements (RE), which in some cases also function as p53 RE. Indeed, many of the p53 RE involved in DNA damage-induced cell cycle arrest or apoptosis are constitutively occupied by ΔNp63 in proliferating keratinocytes [7274] (A.C., unpublished results). Regulation of binding to these elements and changes in the transcriptional capabilities of ΔNp63 are thought to play a role in promoting the exit from the cell cycle of keratinocytes at the onset of their differentiation.

ΔNp63 can control distinct transcriptional networks depending on the state of maturation of keratinocyte precursors, which in turn is dependent on a variety of extracellular stimuli. In proliferating keratinocytes of the basal layers, ΔNp63 can control the expression of basal layer keratins (K5, K14), of molecules required for the formation of the epidermal barrier, such as Alox12 [75], and inhibit proliferation-induced activation of cell cycle arrest genes by competing with p53 for the same responsive elements. Following a differentiation stimulus, ΔNp63 can change its transcriptional activity, detach from the promoter of cell cycle arrest genes (e.g., 14-3-3 sigma and p21waf1), activate genes required for cell cycle exit (IKKa and IRF6), and reorganize the transcription of adhesion molecules to allow keratinocytes to leave the basal layer and stratify (see Figure 1). Differences in the temporal expression, isoform combination, biochemical properties, and transcription activity of p63 protein(s) can have profound impact on the set of genes being transcribed, at a given time in a given cell. This notion implies that during development, p63 protein(s) exert distinct roles, in a time and region-specific manner, an issue that will be resolved only with the generation of isoform-specific knockout or knockdown animals and the analysis of their phenotypes.

Figure 1
Schematic representation of known and proposed p63 pathways relevant for epidermal differentiation, ectoderm-mesoderm signaling, and the onset of ectodermal dysplasias. p63, IKKα, and IRF6 play a role in the developing epidermis, in a cell autonomous ...

Initial approaches to identify p63 targets used vectors to overexpress TA- or ΔN-p63 isoforms in cultured cell lines. Ectopic expression of TAp63 in Ptk2, HR9, F9 cell lines, or in lung epithelial cells induced K14 expression [76, 77]. In contrast ΔN isoforms appear to have an inhibitory role in keratinocyte differentiation, while also inducing K14 expression [64, 78]. These studies have clear limits: they cannot monitor cell-cell (epithelial-mesenchymal) interactions, tissue organization and stratification, but they can only reveal the expression of marker genes. More informative approaches have been employed to identify true TA- and ΔN-p63-specific targets by directly examining keratinocyte progenitor cells, with the added possibility to compare normal keratinocyte progenitors with ones derived from EEC patients or from animal models with p63 mutations. Compared to studying the skin as a tissue (i.e., in vivo or in organ-type cultures), this approach is more likely to yield results relevant for skin development/maturation, as compared to using tumour or immortalized cells. A combination of isoform-specific siRNA-mediated downregulation in primary keratinocytes and in vivo, coupled to analysis in knockout and disease-specific knockin mice, has led to identify key target genes required for epidermal morphogenesis that are involved in pathogenesis of p63-linked ED [11, 54, 55, 79, 80]. The gene coding for the protein kinase IKKα is a transcriptional target of ΔNp63, and indeed ΔNp63 mutant proteins found in EEC are unable to activate IKKα expression. IKKα is a component of the IkB kinase complex and is required for correct epidermal development and epithelial-mesenchymal interaction during development. Recent literature suggests a link between p63 and NFkB [81]; however, the kinase activity of IKKα is not required for its developmental function [40].

IKKα null mice display defects in epidermal, limb, and craniofacial development that are fully reverted after the reexpression of IKKα in the developing ectoderm [40]. Interestingly, IKKα was recently found to be a component of the TGFβ pathway in keratinocytes [82, 83] and to repress FGF8 expression [40]. These observations link ΔNp63 function to the control of developmental signals (TGFβ and FGF8) regulating epidermal, limb, and craniofacial development (see Figure 1).

Similarly, IRF6, another ΔNp63 target gene, is involved in both epidermal development and limb/craniofacial development [55, 84]. The underlying mechanism relates to the ability of IRF6 to modify the stability of the ΔNp63 protein. IRF6 expression is required at the onset of terminal differentiation to allow proteasome-dependent degradation of ΔNp63. Mutations of IRF6 cause syndromes characterized by CL/P and other developmental anomalies, and IRF6 knock-in mice carrying the same mutation found in VWL patients (next paragraph) display a hyperproliferative epidermis that is unable to terminally differentiate [85].

In summary, IKKα and IRF6 are ΔNp63 targets and represent members of a regulated network that control stratification and terminal differentiation of the developing epidermis and also essential in the control of signalling from ectodermal cells to the mesoderm for the correct development of craniofacial structures and limbs. Finally, members of the BMP/TGFβ and FGF families should be regarded as important soluble mediators of this complex regulatory network [84].

6. The Role of p63 in Palate Development

CL/P is a common feature in p63-linked syndromes that is thought to be related to alterations of a tightly controlled balance between proliferation and differentiation of precursor cells during ectoderm development [24]. Since p63 is a transcription factor, the basis of these defects logically resides in the inability of mutated p63 proteins to properly activate/repress the expression of target genes.

We [55] and others [84] have recently discovered that IRF6 is a direct p63 target gene needed for palate development and skin differentiation. IRF6 is a member of a family of interferon-dependent transcription factors [86] that control the proliferation-differentiation switch in epidermal cells [85, 87, 88]. IRF6 is also required for palate closure: mutations in IRF6 are linked to a set of syndromes related to ectodermal dysplasia [89], such as the Van der Woude syndrome (VWS, MIM 119300), an autosomal dominant disorder characterized by CL/P and dental anomalies, and the popliteal pterygium syndrome (MIM 119500) which, in addition to an orofacial phenotype similar to VWS, also displays syndactyly and ankyloblepharon [87, 90]. VWS is the most common CL/P syndrome, accounting for approximately 2% of all cases.

Importantly, the p63 null, the p63-R279H, and the Irf6-R84C homozygous mice all display severe CL/P [55, 84, 85]. The phenotype observed in Irf6 null mice is due to the inability of Irf6 mutant cells to exit the cell cycle, leading to an undifferentiated hyperplastic skin [85, 87]. How this phenotype is linked to p63 is not totally clear; interestingly we noted that ΔNp63 is upregulated in the epidermis of Irf6 null mice. Based on these findings, we propose the existence of a feedback regulatory loop between Irf6 and p63, in which p63 controls Irf6 transcriptionally, while Irf6 controls p63 at the protein-stability level. Importantly, these findings provide a molecular link connecting the IRF6- and p63-linked syndromes [55].

7. p63, Ectoderm Cell Layering and the Control of Limb Development

p63, Dlx5;Dlx6, and FGF8 are coexpressed in the Apical Ectodermal Ridge (AER) of the mouse embryonic limb buds [35] as well as in the fins of the zebrafish embryos [6, 60]. The AER is a transitory ectodermal structure that rims the distal tip of the developing limbs, at the dorsal-ventral border, and is strictly required for limb bud expansion and morphogenesis, in particular for distal outgrowth and digit formation [9193]. Recent models propose that signaling from the AER controls the generation of mesenchymal progenitors, in an instructive way [61, 94, 95]. The best characterized signals emanating from the AER cells are the FGFs, primarily FGF8, which is considered the key AER-derived instructive molecules driving proximo-distal morphogenesis of the limbs [41, 94, 96]. A complex network of reciprocal regulations between Wnt, FGF, and BMPs appears to be at the basis of the coordinated growth of the limb, resulting in time- and location-specific induction of subpopulation of skeletogenic progenitors [61, 91, 97, 98].

The AER is perhaps the first attempt of the embryonic (nonneural) ectoderm to organize into a multilayered epithelial tissue [93]. Considering that p63 has been shown to be required for epidermal stratification [10, 11, 99], it is not surprising that the AER of p63 null or p63 R279H homozygous mice fails to organize as multilayer, in fact in the absence of functional p63 AER formation is nearly prevented. There is experimental evidence to indicate that a failure to maintain the AER is the main pathogenic mechanism in the onset of the ectrodactyly phenotype [93, 100]. In the p63, the Dlx5;Dlx6, and the Dac mutant mice (to name a few), the AER fails to express FGF8 and appears poorly stratified. Thus, loss of AER stratification and reduced FGF8 expression, whether induced by p63 mutation or other genetic conditions, appear to be a common theme during the onset of this specific class of malformations. When FGFR2 gene is deleted in the AER cells, via conditional genetics, the AER loses stratification and FGF8 expression. In this case, the AER cells cannot respond to (AER-derived?) FGFs [94], that are apparently needed for AER maintenance. This is a strong indication that FGF signaling is needed by the AER cells to maintain stratification and function, apparently in an autocrine loop. It is important to note that loss of FGF8 expression alone is not sufficient to explain the loss of AER stratification; however, we should consider that the reduced FGF8 expression seen in SHFM is accompanied by altered expression of several other genes, that may exacerbate the suffering of the AER cells and result in reduced layering.

How is AER stratification controlled by p63? The activity of p63 is increasingly being linked to transcriptional regulation of molecules involved in cell adhesion [101]. Indeed, p63 has been shown to (directly or indirectly) control the expression of EGF-receptor, ICAM, β4-integrin, and Claudin1 [3, 102105]. Furthermore, the p53 responsive transmembrane protein Perp has been implicated in cell-cell adhesion and in the maintenance of epithelial integrity. Perp, a p63 target gene, is also positively regulated by both TA- and ΔN-p63 isoforms, and Perp null mice exhibit blistered stratified epithelium, likely due to compromised adhesion [106]. Recently P-cadherin (CDH3 in human) has been shown to be a transcriptional target of p63 [37], and P-cadherin is the disease gene for the EEM syndrome [26, 27]. However, no limb developmental functions of P-cadherin have been recognized in mice [28], and therefore we currently lack a suitable animal model.

The link between altered adhesion properties and loss of stratification is not totally clear, although the capacity of ectodermal cells to form a multilayered epithelium certainly requires specific adhesion functions, distinct from the single-layer naïve ectoderm. A “cadherin switch” model has been proposed to explain how cell-cell contact may potentially facilitate cell movement and layering [107]. It will be interesting to define how changes in p63 affect this network in a global way.

8. Do p63-Linked Pathways Converge on p63 to Cause Limb Anomalies?

Expression of FGF8 is strongly reduced in the AER of the p63 null, R279H p63 mutant, and Dlx5;Dlx6 mutant embryos [33, 34], as well as several other mouse models of limb defects. A number of observations suggest that the p63 and the Dlx proteins may regulate FGF8 expression by acting directly on the genomic region corresponding to the SHFM-III critical region [37, 108]: indeed true p63-binding sites are present within the region, as demonstrated by ChIP-seq screening [36], and several predicted Dlx binding sites cluster around the FGF8 locus, in genomic regions conserved across mammalian species (see Supplementary Figures  1(a) and 1(b) available online at doi:10.1155/2011/864904). Assuming that Dactylin is not the disease gene for SHFM-III, then FGF8 and components of the NFkB pathway might be the ones. It is tempting to speculate that the complex duplication-rearrangement modifies the position/organization of cis-acting control elements, which in turn may affects expression of FGF8 and components of the NFkB pathway. Thus, in several ectrodactyly mouse models, downregulation of FGF8 appears to be a common feature.

Another regulator of FGF8 expression is the transcription factor Sp8. Animals null for Sp8 show severe limb defects affecting the distal portion of the limbs, associated with a strongly reduced expression of FGF8 [109111]. Sp8 is coexpressed with Dlx genes in the murine AER and forebrain [112] and appears in the top 1% of a list of conserved/coexpressed genes in microarray data (the CLOE algorithm [113, 114]; Dlx binding sites are also predicted in conserved regions near the Sp8 locus (Supplementary Figure  1(c)). Therefore, Sp8 is likely to be a Dlx target and to modulate FGF8 expression.

Another pathway that controls FGF8 expression links p63 with IKKα, a target of p63 relevant for ectoderm development and limb morphogenesis [54, 83, 115]. Interestingly, while mutations of p63 and loss of Dlx5;Dlx6 lead to a reduced FGF8 expression in the AER, IKKα mutant embryos, the AER shows an increase of FGF8 expression [40], a condition that nevertheless results in distal limb truncations and severe malformations.

From the above considerations, it appears that numerous players in the p63 network contribute to regulate FGF8 expression in the AER. FGF8 is dynamically required for the correct establishment of signaling loops within the limb bud [61]—hence for normal limb development. Alterations in FGF8 expression are closely linked to the onset of limb defects and malformations in several mouse models. The severity and extent of the malformation depends much on the time of onset of the AER deficit and the extent of (global) FGF reduction (including FGF4, −9, and −17), as indicated by recently reported results using mice with progressive and combined loss of single and multiple FGF genes [95]. Reduced FGF8 expression and signaling is also closely linked to conditions that alter the AER morphology (reduced layering or altered adhesion). It is important to note that the AER of the AER-specific FGF8 knock-out mice seems morphologically normal [38, 41, 116, 117]. We should also note, however, that in SHFMs the reduced FGF8 expression is always accompanied by altered expression of several other genes.

The possibility that FGF8 is a common target of p63 network during limb development is in agreement with the well-known functions of FGF8 to sustain epithelial-mesenchymal signalling and assure the timely generation of the correct population of mesenchymal progenitors [95]. Should this hypothesis be true, this knowledge could be used in preclinical studies on mouse models, to attempt to restore sufficient levels of FGF exogenously, and hope to rescue normal limb development.

9. Dynamic Gene Expression of Partially Redundant Genes Is Critical for the Activity of p63 and the Onset of Disease Phenotypes

An emerging theme in developmental biology is the importance of gene dosage and dynamic gene expression for correct morphogenesis [98]. Notable examples of this are the signaling functions of FGFs expressed in the AER [95], the gene-dosage-dependent functions of Msx1 and Msx2 for osteogenic differentiation of cranial neural crest cells [118], the progressive limb phenotypes and altered Epha3 expression associated with the loss of posterior HoxD alleles [119], and the craniofacial phenotypes of embryos mutant for the Edn1-Dlx pathway [120]. Recent studies nicely illustrate the concept of “relativity of gene function”, in particular during limb development [91]. In fact, early or late gene inactivation or misexpression can profoundly change the phenotypic outcome.

Consequently, such dynamic changes in gene functions may escape detection when genetic analysis is limited to constitutively null allele. On the same note, the function of individual genes is best examined upon partial and cumulative gene losses, and within the context of expression of related genes, as for example has been done in [95].

Several Dlx (1, 2, 3, 5, and 6) and FGF (4, 8, 9, and 17), genes are coexpressed in the AER, and their expression is dynamically regulated, both in respect with time (embryonic age) and location (territory of expression). In addition, there is evidence that Dlx and FGF genes are functionally redundant, at least in part. For example, no limb phenotype is observed in mice null for only one Dlx gene, while an ectrodactyly phenotype is observed in Dlx2;Dlx5 null mice [121]. Furthermore, the ectrodactyly seen in the Dlx5;Dlx6 mutant mice is fully rescued by the reexpression of only Dlx5 [34]. An increased severity of craniofacial phenotypes correlates with progressive loss of more than one Dlx gene [120, 122]. Likewise, FGF8 and FGF4 represent the principal supply of FGF from the AER [38, 41], and FGF4 could functionally replace FGF8 [123]. All these are indication of a gene-dosage effect between functionally redundant genes.

We propose that the portion of the p63 network that (direct or indirect) regulates FGF8 expression is exerted in a quantitative and dynamic mode. To support this, we should consider that although p63 null and p63EEC homozygous mice show severe limb truncation or absence, the heterozygous mice appear to be normal. When heterozygous EEC mice are crossed with heterozygous Dlx5;Dlx6 ones (also with apparently normal limbs), clear anomalies are observed, although mild [35].

A gene-dosage effect combined with the coexpression of functionally redundant genes implies the existence of a threshold level to be maintained to assure AER stratification and signaling functions. Following this logic, we have determined the expression of Dlx genes along the antero-posterior AER, by qPCR, and have noted that the expression of Dlx2 and Dlx5 is lower in the central portion of the AER, compared to the anterior or posterior segments. This may explain why in the absence of Dlx5;Dlx6 only the central ray of the limb bud is affected: the central AER might be more sensitive to reduced Dlx expression due to intrisnic lower expression, and the loss of two or more Dlx gene may drop the level of pan-Dlx below the threshold.

On the same line, there is evidence that a certain amount of AER-derived pan-FGF is required to induce and maintain the underlying mesenchymal progenitors [61, 93, 95]. In fact, in the Dlx5;Dlx6 DKO limbs, the reduction of FGF8 expression is restricted to the central AER, the region where epithelial-mesenchymal signaling is primarily defective and the region where morphogenesis fails [33, 34]. Thus, the entire p63-Dlx-FGF is sensitive to gene dosage, timing, and position.

On the same note, we have determined the relative expression of Dlx genes comparing the FL and the HL at the same embryonic age, by qPCR. The results indicate that in the HL expression is generally lower (−15–20%) than that in the FL (Figure 3), supporting the relevance of dynamic expression for developmental defects. This may explain the finding that the HLs are usually more severely affected than the FLs. It is well known that the initiation and growth of the HL lags behind that of the FL [93]. Similarly, when FGFR2 is conditionally deleted in the AER, the HLs are less severely affected then the FLs. In these mice, the expression of FGF8 is first lost in the central wedge of the limb bud and this is associated with loss of stratification [94]. Thus, different dynamics of gene expression result in distinct phenotypic outcomes.

Figure 3
Quantitative and dynamic expression of Dlx genes during limb development. (a) Expression of Dlx genes in the hindlimbs (HL) and forelimbs (FL) limbs, at the same embryonic age, by qPCR. In the HL, the expression is always lower, as compared to the ...

10. Emerging p63 Regulatory Pathways—A Summary

Classical strategies have been adopted to search for phenotype-relevant p63 targets by “candidate gene” approaches or by genome-wide screenings. More modern approaches include the elaboration of a Position Weight Matrix combined with promoter occupancy data. It is expected that in the near future a wealth of high-throughput data (expressed genes and microRNA profiles, ChIP-seq, histone modification map) will be collected and new opportunities will emerge from meta-analyses of these complex data. In this direction, recently published work [36] reports the ChIP-seq data for p63 obtained from cultured keratinocytes. We should soon be able to define an evidence-based p63-network and thus raise novel hypotheses towards the identification of converging pathways and key players amenable to interventions. Here we summarize regulatory links that have either been demonstrated or appear highly likely and the supporting evidence (Figure 2).

Figure 2
Schematic representation of known and proposed p63 pathways relevant for limb development and the onset of ectrodactyly. P-cadherin is a known disease gene only in human, while Dlx5;Dlx6 are known disease genes only in mice. Dactylin has been proposed ...

10.1. p63 Upstream of Ikkα

Ikka is a transcriptional target of p63 [54, 83, 115]. Ikkα null mice show malformations of the limb skeleton and abnormal epidermal differentiation. Surprisingly, in the absence of Ikkα the expression of FGF8 is upregulated, indicating that any variation in FGF8 level is deleterious for the ectoderm-derived cells [40].

10.2.p63 Upstream of Dlx5;Dlx6

Dlx5 and Dlx6 are coexpressed with p63 in the AER, and their expression is diminished in the absence of p63 or in the presence of the R279H homozygous mutation [35]. This regulation occurs by (1) binding on the Dlx5 and Dlx6 promoters and activation of their transcription [35] and (2) distant regulation by an enhancer-like element located 250 kbp upstream of the Dlx6 promoter [36]. Importantly, such p63-responsive enhancer element is deleted in one SHFM patient [36]. Also the expression of Dlx1;Dlx2 is diminished in p63 mutant embryonic limbs, and Dlx1 and Dlx2 are located near the critical region for SHFM-V. If the deletion alters their expression by positional effect and distal enhancers, Dlx1;Dlx2 may turn out to be the SHFM-V disease genes.

10.3. p63 and Dlx5;Dlx6 Upstream of FGF8

Based on Expressed Gene profiling comparing p63-silenced keratinocytes with control ones [55] (A.C. unpublished), and based on recently published ChIP-seq data that identify true p63 binding sites within the SHFM-III critical region [36], there is a justified possibility that p63 regulates FGF8 expression via cis-acting elements. Indeed, FGF8 expression is strongly reduced in the AER of p63 null and p63 R279H mutant embryos. FGF8 expression is also diminished in the AER of Dlx5;Dlx6 mutant embryos [33, 34]. Using a Position Weight Matrix approach to scan conserved regions of the mammalian genome for predicted Dlx binding sites, a high number of conserved Dlx-binding sites is found around the FGF8 locus and in the SHFM-III critical region (Supplementary Figure  1).

10.4. p63 Upstream of Dlx3

Dlx3 codes for a homeodomain transcription factor, member of the distalless family, expressed in keratinocytes [52] and responsible for p63  degradation during their differentiation [69, 70]. A negative feedback regulation between p63 and Dlx3 has recently been uncovered, that seems to be responsible for the TDO syndrome [124].

10.5. p63 Upstream of P-Cadherin

The P-cadherin gene (CDH3 in human) has been shown to be a transcriptional target of p63 [27]. Interestingly, P-cadherin is mutated in the EEM syndrome, characterized by the presence of the SHFM phenotype [26, 27]. However, no limb developmental functions of P-cadherin have been shown in mice [28], and therefore the role of this molecule remains unclear.

10.6. Dlx5;Dlx6 Upstream of Wnt5a

Several observations suggest that Wnt5a is likely to be a transcriptional target of Dlx genes. First, Wnt5a expression is reduced in the AER of Dlx5;Dlx6 mutant limbs (G.M. and LoIacono, unpublished), and Dlx2 and Dlx5 directly bind to regulatory elements in the Wnt5a locus and modulate transcription of Wnt5a in neural progenitors [125]. Second, Wnt5a null embryos exhibit a severe limb phenotype characterized by truncations of proximal elements and absence of the fingers, although the AER appears normal and expresses FGF8 [126]. Third, D-Wnt5 is a target of distalles in the Drosophila limbs [127]. Wnt5a is a short-range signaling molecule that could participate in a network of epithelial-mesenchymal signaling together with FGFs to induce and maintain specific pools of mesenchymal progenitors, as recently proposed [97]. One interesting possibility is that the activity of the “noncanonical” Wnt5a might antagonize the activity of “canonical” Wnts [128], known to be required for AER maintenance and limb morphogenesis [129132].

11. Conclusions and Perspectives

Isoform-specific p63 transcriptional networks are being defined that begin to reveal the molecular basis for the dual function of this protein: (a) maintain the stem state of epidermal progenitors and (b) assure that cells can escape the stem state, exit the cell cycle, stratify and terminally differentiate. In the embryonic ectoderm, these apparently conflicting activities are strongly biased towards the maintenance of the stem state, while during subsequent development a finely-tuned equilibrium needs to be established to sustain turn-over, regeneration, and differentiation. In EEC patients, the presence of one mutated p63 allele generates a condition in which this equilibrium is compromised, and an altered progenitor-maintenance function ensues and results in a dysplastic skin. In order to further comprehend the role of p63 at the tissue level, mice null for p63 appear not to be the ideal model, as both the progenitor maintenance and the cell cycle escape functions are simultaneously compromised due to the total absence of the protein. Better animal models are therefore needed, such as isoform-specific knock-outs or knock-in of point mutated alleles. As today, the EEC and the AEC p63 mouse models appear to better recapitulate the human diseases and should therefore be used more extensively.

The Apical Ectodermal Ridge (AER) is a region of the embryonic ectoderm specialized in signaling functions and responsible for outgrowth and patterning of the limbs. This function is exerted mostly via FGF signaling. The AER is perhaps the earliest attempt of ectodermal cells to organize into a multilayered tissue. Considering that p63 has been directly implicated in keratinocyte stratification, it is not surprising that the limb defects seen in EEC and related disorders consistently show loss of AER stratification, associated with reduced FGF8 expression. Here we raise and justify the hypothesis that FGF8 might be the converging molecules on which various limb morphogenetic pathways centered on p63 impinge, directly or indirectly. We also present and discuss those indications suggesting that the AER-expressed FGFs and the Dlx genes act in a dose-dependent fashion and that their expression is dynamically regulated. Such “quantitative” effects have an influence on the establishment of correct signalling within the developing limb and could explain some features of the limb anomalies.

Recently published findings and unpublished results point to the importance of degradation of ΔNp63 during epidermis differentiation. This critical function appears to be exerted by at least three molecules (Dlx3, IRF6, Itch), although additional p63 degradation pathways are likely to emerge. In the near future, all aspects of the p63 upstream and downstream networks will be further clarified and initial efforts in this direction suggest the existence of an intricate network of regulations [133, 134].

Deciphering and comprehending the complete p63 network underlying cellular-developmental defects affecting ectoderm derivatives is the next critical task, expected to yield relevant new knowledge on the components of this network and on their regulation. Transcription profiling done on homogeneous cell populations and well-designed comparisons, have certainly been useful. However, for adult tissues or embryonic structures this approach is problematic and not easy to apply; furthermore, there are no cultured cell lines that can faithfully reproduce cell layering, “quantitative” gene expression, and dynamic signaling as they occur in the intact skin, palatal shelf, or limb bud.

Thus, scientist will engage in scientific activities that combine phenotype-causing targeted mutations followed by reexpression of a candidate target in vivo to monitor aggravation or correction of the developmental phenotype. In the case of the p63-Dlx regulation, this approach has been informative, and other best-candidates for being p63 and Dlx5;Dlx6 targets should likewise be tested. The in vivo approach is preferable, although time consuming, since p63 and most of the upstream and downstream players are express in a tissue-specific way and/or they are involved or depend on tissue interactions and signalling, notoriously difficult to be recapitulated in vitro. Emerging targets are IRF6, IKKα (for the epidermis, palate, and limbs), Wnt5a, and FGF8 (for the limbs), and important new discoveries are expected in this direction.

The long-term hope is to identify key enzymes or a ligand/receptor signaling systems, to be used to test the activity of exogenously provided ligands or active compounds in preclinical experimental setting, perhaps on skin, limb or palate organ-type cultures, and hope to revert the dysplastic/malformation phenotypes.


The authors thank Giulia Garaffo and Paolo Provero (University of Torino) for sharing unpubished results and bioinformatic predictions. They also thank Dr. Alea A. Mills (Cold Spring Harbor Lab. USA) for sharing unpublished observations on the p63-R279H mice and Stefano Mantero (Telethon Laboratory, University of Torino) for the qPCR data on Dlx expression. They are grateful to Drs. P. P. Pandolfi and E. Calautti (University of Torino) for comments and criticism regarding the paper.


1. Ghioni P, Bolognese F, Duijf PHG, Van Bokhoven H, Mantovani R, Guerrini L. Complex transcriptional effects of p63 isoforms: identification of novel activation and repression domains. Molecular and Cellular Biology. 2002;22(24):8659–8668. [PMC free article] [PubMed]
2. Mangiulli M, Valletti A, Caratozzolo MF, et al. Identification and functional characterization of two new transcriptional variants of the human p63 gene. Nucleic Acids Research. 2009;37(18):6092–6104. [PMC free article] [PubMed]
3. Yang A, Zhu Z, Kapranov P, et al. Relationships between p63 binding, DNA sequence, transcription activity, and biological function in human cells. Molecular Cell. 2006;24(4):593–602. [PubMed]
4. Thanos CD, Bowie JU. p53 Family members p63 and p73 are SAM domain-containing proteins. Protein Science. 1999;8(8):1708–1710. [PubMed]
5. Serber Z, Lai HC, Yang A, et al. A C-terminal inhibitory domain controls the activity of p63 by an intramolecular mechanism. Molecular and Cellular Biology. 2002;22(24):8601–8611. [PMC free article] [PubMed]
6. Bakkers J, Hild M, Kramer C, Furutani-Seiki M, Hammerschmidt M. Zebrafish ΔNp63 is a direct target of Bmp signaling and encodes a transcriptional repressor blocking neural specification in the ventral ectoderm. Developmental Cell. 2002;2(5):617–627. [PubMed]
7. Koster MI, Roop DR. p63 and epithelial appendage development. Differentiation. 2004;72(8):364–370. [PubMed]
8. Koster MI, Roop DR. Transgenic mouse models provide new insights into the role of p63 in epidermal development. Cell Cycle. 2004;3(4):411–413. [PubMed]
9. Koster MI, Roop DR. The role of p63 in development and differentiation of the epidermis. Journal of Dermatological Science. 2004;34(1):3–9. [PubMed]
10. Koster MI, Kim S, Mills AA, DeMayo FJ, Roop DR. p63 is the molecular switch for initiation of an epithelial stratification program. Genes and Development. 2004;18(2):126–131. [PubMed]
11. Koster MI, Roop DR. Mechanisms regulating epithelial stratification. Annual Review of Cell and Developmental Biology. 2007;23:93–113. [PubMed]
12. Laurikkala J, Mikkola ML, James M, Tummers M, Mills AA, Thesleff I. p63 regulates multiple signalling pathways required for ectodermal organogenesis and differentiation. Development. 2006;133(8):1553–1563. [PubMed]
13. Finlan LE, Hupp TR. p63: the phantom of the tumor suppressor. Cell Cycle. 2007;6(9):1062–1071. [PubMed]
14. Tomkova K, Tomka M, Zajac V. Contribution of p53, p63, and p73 to the developmental diseases and cancer. Neoplasma. 2008;55(3):177–181. [PubMed]
15. Ianakiev P, Kilpatrick MW, Toudjarska I, Basel D, Beighton P, Tsipouras P. Split-hand/split-foot malformation is caused by mutations in the p63 gene on 3q27. American Journal of Human Genetics. 2000;67(1):59–66. [PubMed]
16. Brunner HG, Hamel BCJ, Van Bokhoven H. P63 gene mutations and human developmental syndromes. American Journal of Medical Genetics. 2002;112(3):284–290. [PubMed]
17. Brunner HG, Hamel BCJ, Van Bokhoven H. The p63 gene in EEC and other syndromes. Journal of Medical Genetics. 2002;39(6):377–381. [PMC free article] [PubMed]
18. Van Bokhoven H, Brunner HG. Splitting p63. American Journal of Human Genetics. 2002;71(1):1–13. [PubMed]
19. Van Bokhoven H, McKeon F. Mutations in the p53 homolog p63: allele-specific developmental syndromes in humans. Trends in Molecular Medicine. 2002;8(3):133–139. [PubMed]
20. Van Bokhoven H, Hamel BCJ, Bamshad M, et al. p63 gene mutations in EEC syndrome, limb-mammary syndrome, and isolated split hand-split foot malformation suggest a genotype-phenotype correlation. American Journal of Human Genetics. 2001;69(3):481–492. [PubMed]
21. Celli J, Duijf P, Hamel BCJ, et al. Heterozygous germline mutations in the p53 homolog p63 are the cause of EEC syndrome. Cell. 1999;99(2):143–153. [PubMed]
22. Rinne T, Hamel B, Van Bokhoven H, Brunner HG. Pattern of p63 mutations and their phenotypes—update. American Journal of Medical Genetics, Part A. 2006;140(13):1396–1406. [PubMed]
23. Elliott AM, Evans JA, Chudley AE. Split hand foot malformation (SHFM) Clinical Genetics. 2005;68(6):501–505. [PubMed]
24. Rinne T, Brunner HG, Van Bokhoven H. p63-associated disorders. Cell Cycle. 2007;6(3):262–268. [PubMed]
25. Ugur SA, Tolun A. Homozygous WNT10b mutation and complex inheritance in Split-Hand/Foot Malformation. Human Molecular Genetics. 2008;17(17):2644–2653. [PubMed]
26. Kjaer KW, Hansen L, Schwabe GC, et al. Distinct CDH3 mutations cause ectodermal dysplasia, ectrodactyly, macular dystrophy (EEM syndrome) Journal of Medical Genetics. 2005;42(4):292–298. [PMC free article] [PubMed]
27. Shimomura Y, Wajid M, Shapiro L, Christiano AM. P-cadherin is a p63 target gene with a crucial role in the developing human limb bud and hair follicle. Development. 2008;135(4):743–753. [PubMed]
28. Radice GL, Ferreira-Cornwell MC, Robinson SD, et al. Precocious mammary gland development in P-cadherin-deficient mice. Journal of Cell Biology. 1997;139(4):1025–1032. [PMC free article] [PubMed]
29. Del Porto G, D’Alessandro E, De Matteis C, Lo Re ML, Ivaldi M, Di Fusco C. Interstitial deletion of the long arm of chromosome 7 and its clinical correlationsDelezione interstiziale del braccio lungo del cromosoma 7 e sue correlazioni cliniche. Pathologica. 1983;75:268–271. [PubMed]
30. Marinouni JC, Stevenson RE, Evans JP, Geshuri D, Phelan MC, Schwartz CE. Split foot and developmental retardation associated with a deletion of three microsatellite markers in 7q21.2-q22.1. Clinical Genetics. 1995;47(2):90–95. [PubMed]
31. Scherer SW, Cheung J, MacDonald JR, et al. Human chromosome 7: DNA sequence and biology. Science. 2003;300(5620):767–772. [PMC free article] [PubMed]
32. Acampora D, Merlo GR, Paleari L, et al. Craniofacial, vestibular and bone defects in mice lacking the Distal-less-related gene Dlx5. Development. 1999;126(17):3795–3809. [PubMed]
33. Merlo GR, Paleari L, Mantero S, et al. Mouse model of split hand/foot malformation type I. Genesis. 2002;33(2):97–101. [PubMed]
34. Robledo RF, Rajan L, Li X, Lufkin T. The D1x5 and D1x6 homeobox genes are essential for craniofacial, axial, and appendicular skeletal development. Genes and Development. 2002;16(9):1089–1101. [PubMed]
35. Iacono NL, Mantero S, Chiarelli A, et al. Regulation of Dlx5 and Dlx6 gene expression by p63 is involved in EEC and SHFM congenital limb defects. Development. 2008;135(7):1377–1388. [PubMed]
36. Kouwenhoven EN, va Heeringen SJ, Tena JJ, et al. Genome-wide profiling of p63 DNA-binding sites identifies an element that regulates gene expression during limb development in the 7q21 shfm1 locus. PLoS Genetics. 2010;6(8) Article ID e1001065. [PMC free article] [PubMed]
37. de Mollerat XJ, Gurrieri F, Morgan CT, et al. A genomic rearrangement resulting in a tandem duplication is associated with split hand-split foot malformation 3 (SHFM3) at 10q24. Human Molecular Genetics. 2003;12(16):1959–1971. [PubMed]
38. Boulet AM, Moon AM, Arenkiel BR, Capecchi MR. The roles of Fgf4 and Fgf8 in limb bud initiation and outgrowth. Developmental Biology. 2004;273(2):361–372. [PubMed]
39. Bushdid PB, Brantley DM, Yull FE, et al. Inhibition of NF-κB activity results in disruption of the apical ectodermal ridge and aberrant limb morphogenesis. Nature. 1998;392(6676):615–618. [PubMed]
40. Sil AK, Maeda S, Sono Y, Roop DB, Karin M. IκB kinase-α acts in the epidermis to control skeletal and craniofacial morphogenesis. Nature. 2004;428(6983):660–664. [PubMed]
41. Sun X, Mariani FV, Martin GR. Functions of FGF signalling from the apical ectodermal ridge in limb development. Nature. 2002;418(6897):501–508. [PubMed]
42. Del Campo M, Jones MC, Veraksa AN, et al. Monodactylous limbs and abnormal genitalia are associated with hemizygosity for the human 2q31 region that includes the HOXD cluster. American Journal of Human Genetics. 1999;65(1):104–110. [PubMed]
43. Goodman FR, Majewski F, Collins AL, Scambler PJ. A 117-kb microdeletion removing HOXD9-HOXD13 and EVX2 causes synpolydactyly. American Journal of Human Genetics. 2002;70(2):547–555. [PubMed]
44. Goodman FR. Limb malformations and the human HOX genes. American Journal of Medical Genetics. 2002;112(3):256–265. [PubMed]
45. Faiyaz-Ul-Haque M, Zaidi SHE, King LM, et al. Fine mapping of the X-linked split-hand/split-foot malformation (SHFM2) locus to a 5.1-Mb region on Xq26.3 and analysis of candidate genes. Clinical Genetics. 2005;67(1):93–97. [PubMed]
46. Lim J, Hao T, Shaw C, et al. A protein-protein interaction network for human inherited ataxias and disorders of Purkinje cell degeneration. Cell. 2006;125(4):801–814. [PubMed]
47. Oti M, Huynen MA, Brunner HG. The biological coherence of human phenome databases. American Journal of Human Genetics. 2009;85(6):801–808. [PubMed]
48. Tidyman WE, Rauen KA. The RASopathies: developmental syndromes of Ras/MAPK pathway dysregulation. Current Opinion in Genetics and Development. 2009;19(3):230–236. [PMC free article] [PubMed]
49. Priolo M. Ectodermal dysplasias: an overview and update of clinical and molecular-functional mechanisms. American Journal of Medical Genetics, Part A. 2009;149(9):2003–2013. [PubMed]
50. Mills AA, Zheng B, Wang XJ, Vogel H, Roop DR, Bradley A. p63 is a p53 homologue required for limb and epidermal morphogenesis. Nature. 1999;398(6729):708–713. [PubMed]
51. Yang A, Schweitzer R, Sun D, et al. p63 is essential for regenerative proliferation in limb, craniofacial and epithelial development. Nature. 1999;398(6729):714–718. [PubMed]
52. Radoja N, Guerrini L, Iacono NL, et al. Homeobox gene Dlx3 is regulated by p63 during ectoderm development: relevance in the pathogenesis of ectodermal dysplasias. Development. 2007;134(1):13–18. [PubMed]
53. Mikkola ML, Costanzo A, Thesleff I, Roop DR, Koster MI. Treasure or artifact: a decade of p63 research speaks for itself. Cell death and differentiation. 2010;17(1):180–183. [PMC free article] [PubMed]
54. Marinari B, Ballaro C, Koster MI, et al. IKKalpha is a p63 transcriptional target involved in the pathogenesis of ectodermal dysplasias. The Journal of Investigative Dermatology. 2009;129(1):60–69. [PubMed]
55. Moretti F, Marinari B, Iacono NL, et al. A regulatory feedback loop involving p63 and IRF6 links the pathogenesis of 2 genetically different human ectodermal dysplasias. Journal of Clinical Investigation. 2010;120(5):1570–1577. [PMC free article] [PubMed]
56. Koster MI, Marinari B, Payne AS, Kantaputra PN, Costanzo A, Roop DR. ΔNp63 knockdown mice: a mouse model for AEC syndrome. American Journal of Medical Genetics, Part A. 2009;149(9):1942–1947. [PMC free article] [PubMed]
57. Chai CK. Dactylaplasia in mice. A two-locus model for developmental anomalies. Journal of Heredity. 1981;72(4):234–237. [PubMed]
58. Johnson KR, Lane PW, Ward-Bailey P, Davisson MT. Mapping the mouse dactylaplasia mutation, Dac, and a gene that controls its expression, mdac. Genomics. 1995;29(2):457–464. [PubMed]
59. Crackower MA, Motoyama J, Tsui LC. Defect in the maintenance of the apical ectodermal ridge in the Dactylaplasia mouse. Developmental Biology. 1998;201(1):78–89. [PubMed]
60. Lee H, Kimelman D. A dominant-negative form of p63 is required for epidermal proliferation in zebrafish. Developmental Cell. 2002;2(5):607–616. [PubMed]
61. Zeller R, López-Ríos J, Zuniga A. Vertebrate limb bud development: moving towards integrative analysis of organogenesis. Nature Reviews Genetics. 2009;10(12):845–858. [PubMed]
62. Medawar A, Virolle T, Rostagno P, et al. ΔNp63 is essential for epidermal commitment of embryonic stem cells. PLoS One. 2008;3(10) Article ID e3441. [PMC free article] [PubMed]
63. Senoo M, Pinto F, Crum CP, McKeon F. p63 is essential for the proliferative potential of stem cells in stratified epithelia. Cell. 2007;129(3):523–536. [PubMed]
64. King KE, Ponnamperuma RM, Yamashita T, et al. ΔNp63α functions as both a positive and a negative transcriptional regulator and blocks in vitro differentiation of murine keratinocytes. Oncogene. 2003;22(23):3635–3644. [PubMed]
65. Nguyen BC, Lefort K, Mandinova A, et al. Cross-regulation between Notch and p63 in keratinocyte commitment to differentiation. Genes and Development. 2006;20(8):1028–1042. [PubMed]
66. Galli F, Rossi M, D'Alessandra Y, et al. MDM2 and Fbw7 cooperate to induce p63 protein degradation following DNA damage and cell differentiation. Journal of Cell Science. 2010;123(14):2423–2433. [PubMed]
67. Rossi M, Aqeilan RI, Neale M, et al. The E3 ubiquitin ligase Itch controls the protein stability of p63. Proceedings of the National Academy of Sciences of the United States of America. 2006;103(34):12753–12758. [PubMed]
68. Rossi M, De Simone M, Pollice A, et al. Itch/AIP4 associates with and promotes p63 protein degradation. Cell Cycle. 2006;5(16):1816–1822. [PubMed]
69. Di Costanzo A, Festa L, Duverger O, et al. Homeodomain protein Dlx3 induces phosphorylation-dependent p63 degradation. Cell Cycle. 2009;8(8):1185–1195. [PMC free article] [PubMed]
70. Moretti F, Costanzo A. A feedback regulatory loop between p63 and Dlx3: implications for epidermal differentiation. Cell Cycle. 2009;8(8):p. 1113. [PubMed]
71. Yi R, Poy MN, Stoffel M, Fuchs E. A skin microRNA promotes differentiation by repressing ’stemness’ Nature. 2008;452(7184):225–229. [PubMed]
72. Barbieri CE, Pietenpol JA. p53 family members: similar biochemistry, different biology. Cancer Biology and Therapy. 2005;4(4):419–420. [PubMed]
73. Hearnes JM, Mays DJ, Schavolt KL, Tang L, Jiang X, Pietenpol JA. Chromatin immunoprecipitation-based screen to identify functional genomic binding sites for sequence-specific transactivators. Molecular and Cellular Biology. 2005;25(22):10148–10158. [PMC free article] [PubMed]
74. Papoutsaki M, Moretti F, Lanza M, et al. A p38-dependent pathway regulates ΔNp63 DNA binding to p53-dependent promoters in UV-induced apoptosis of keratinocytes. Oncogene. 2005;24(46):6970–6975. [PubMed]
75. Kim S, Choi IF, Quante JR, Zhang L, Roop DR, Koster MI. P63 directly induces expression of Alox12, a regulator of epidermal barrier formation. Experimental Dermatology. 2009;18(12):1016–1021. [PMC free article] [PubMed]
76. Koster MI, Kim S, Huang J, Williams T, Roop DR. TAp63α induces AP-2γ as an early event in epidermal morphogenesis. Developmental Biology. 2006;289(1):253–261. [PubMed]
77. Koster MI, Roop DR. Genetic pathways required for epidermal morphogenesis. European Journal of Cell Biology. 2004;83(11-12):625–629. [PubMed]
78. Romano RA, Birkaya B, Sinha S. A functional enhancer of keratin14 is a direct transcriptional target of ΔNp63. Journal of Investigative Dermatology. 2007;127(5):1175–1186. [PubMed]
79. Beaudry VG, Pathak N, Koster MI, Attardi LD. Differential PERP regulation by TP63 mutants provides insight into AEC pathogenesis. American Journal of Medical Genetics, Part A. 2009;149(9):1952–1957. [PubMed]
80. Koster MI, Dai D, Marinari B, et al. p63 induces key target genes required for epidermal morphogenesis. Proceedings of the National Academy of Sciences of the United States of America. 2007;104(9):3255–3260. [PubMed]
81. Sen T, Chang X, Sidransky D, Chatterjee A. Regulation of ΔNp63α by NFκB. Cell Cycle. 2010;9(24):4841–4847. [PMC free article] [PubMed]
82. Descargues P, Sil AK, Sano Y, et al. IKKα is a critical coregulator of a Smad4-independent TGFβ-Smad2/3 signaling pathway that controls keratinocyte differentiation. Proceedings of the National Academy of Sciences of the United States of America. 2008;105(7):2487–2492. [PubMed]
83. Marinari B, Moretti F, Botti E, et al. The tumor suppressor activity of IKKα in stratified epithelia is exerted in part via the TGF-β antiproliferative pathway. Proceedings of the National Academy of Sciences of the United States of America. 2008;105(44):17091–17096. [PubMed]
84. Thomason HA, Zhou H, Kouwenhoven EN, et al. Cooperation between the transcription factors p63 and IRF6 is essential to prevent cleft palate in mice. Journal of Clinical Investigation. 2010;120(5):1561–1569. [PMC free article] [PubMed]
85. Richardson RJ, Dixon J, Malhotra S, et al. Irf6 is a key determinant of the keratinocyte proliferation-differentiation switch. Nature Genetics. 2006;38(11):1329–1334. [PubMed]
86. Taniguchi T, Takaoka A. A weak signal for strong responses: interferon-α/β revisited. Nature Reviews Molecular Cell Biology. 2001;2(5):378–386. [PubMed]
87. Ingraham CR, Kinoshita A, Kondo S, et al. Abnormal skin, limb and craniofacial morphogenesis in mice deficient for interferon regulatory factor 6 (Irf6) Nature Genetics. 2006;38(11):1335–1340. [PMC free article] [PubMed]
88. Rahimov F, Marazita ML, Visel A, et al. Disruption of an AP-2α binding site in an IRF6 enhancer is associated with cleft lip. Nature Genetics. 2008;40(11):1341–1347. [PMC free article] [PubMed]
89. Little HJ, Rorick NK, Su LI, et al. Missense mutations that cause Van der Woude syndrome and popliteal pterygium syndrome affect the DNA-binding and transcriptional activation functions of IRF6. Human Molecular Genetics. 2009;18(3):535–545. [PMC free article] [PubMed]
90. Kondo S, Schutte BC, Richardson RJ, et al. Mutations in IRF6 cause Van der Woude and popliteal pterygium syndromes. Nature Genetics. 2002;32(2):285–289. [PMC free article] [PubMed]
91. Bénazet JD, Zeller R. Vertebrate limb development: moving from classical morphogen gradients to an integrated 4-dimensional patterning system. Cold Spring Harbor Perspectives in Biology. 2009;1(4) Article ID a001339. [PMC free article] [PubMed]
92. Capdevila J, Belmonte JCI. Patterning mechanisms controlling vertebrate limb development. Annual Review of Cell and Developmental Biology. 2001;17:87–132. [PubMed]
93. Fernandez-Teran M, Ros MA. The Apical Ectodermal Ridge: morphological aspects and signaling pathways. International Journal of Developmental Biology. 2008;52(7):857–871. [PubMed]
94. Lu P, Yu Y, Perdue Y, Werb Z. The apical ectodermal ridge is a timer for generating distal limb progenitors. Development. 2008;135(8):1395–1405. [PMC free article] [PubMed]
95. Mariani FV, Ahn CP, Martin GR. Genetic evidence that FGFs have an instructive role in limb proximal-distal patterning. Nature. 2008;453(7193):401–405. [PMC free article] [PubMed]
96. Sanz-Ezquerro JJ, Tickle C. Digital development and morphogenesis. Journal of Anatomy. 2003;202(1):51–58. [PubMed]
97. ten Berge D, Brugmann SA, Helms JA, Nusse R. Wnt and FGF signals interact to coordinate growth with cell fate specification during limb development. Development. 2008;135(19):3247–3257. [PMC free article] [PubMed]
98. Zeller R. The temporal dynamics of vertebrate limb development, teratogenesis and evolution. Current Opinion in Genetics and Development. 2010;20(4):384–390. [PubMed]
99. Candi E, Cipollone R, Rivetti Di Val Cervo P, Gonfloni S, Melino G, Knight R. p63 in epithelial development. Cellular and Molecular Life Sciences. 2008;65(20):3126–3133. [PubMed]
100. Duijf PHG, van Bokhoven H, Brunner HG. Pathogenesis of split-hand/split-foot malformation. Human Molecular Genetics. 2003;12(1):R51–R60. [PubMed]
101. Carroll DK, Carroll JS, Leong CO, et al. p63 regulates an adhesion programme and cell survival in epithelial cells. Nature Cell Biology. 2006;8(6):551–561. [PubMed]
102. Barbieri CE, Tang LJ, Brown KA, Pietenpol JA. Loss of p63 leads to increased cell migration and up-regulation of genes involved in invasion and metastasis. Cancer Research. 2006;66(15):7589–7597. [PubMed]
103. Lopardo T, Lo Iacono N, Marinari B, et al. Claudin-1 is a p63 target gene with a crucial role in epithelial development. PLoS One. 2008;3(7) Article ID e2715. [PMC free article] [PubMed]
104. Testoni B, Borrelli S, Tenedini E, et al. Identification of new p63 targets in human keratinocytes. Cell Cycle. 2006;5(23):2805–2811. [PubMed]
105. Viganò MA, Lamartine J, Testoni B, et al. New p63 targets in keratinocytes identified by a genome-wide approach. EMBO Journal. 2006;25(21):5105–5116. [PubMed]
106. Ihrie RA, Marques MR, Nguyen BT, et al. Perp is a p63-regulated gene essential for epithelial integrity. Cell. 2005;120(6):843–856. [PubMed]
107. Jamora C, DasGupta R, Kocieniewski P, Fuchs E. Links between signal transduction, transcription and adhesion in epithelial bud development. Nature. 2003;422(6929):317–322. [PMC free article] [PubMed]
108. Sidow A, Bulotsky MS, Kerrebrock AW, et al. A novel member of the F-box/WD40 gene family, encoding dactylin, is disrupted in the mouse dactylaplasia mutant. Nature Genetics. 1999;23(1):104–107. [PubMed]
109. Bell SM, Schreiner CM, Waclaw RR, Campbell K, Pottert SS, Scottt WJ. Sp8 is crucial for limb outgrowth and neuropore closure. Proceedings of the National Academy of Sciences of the United States of America. 2003;100(21):12195–12200. [PubMed]
110. Kawakami Y, Rodríguez-Esteban C, Matsui T, Rodríguez-León J, Kato S, Izpisúa Belmonte JC. Sp8 and Sp9, two closely related buttonhead-like transcription factors, regulate Fgf8 expression and limb outgrowth in vertebrate embryos. Development. 2004;131(19):4763–4774. [PubMed]
111. Treichel D, Schöck F, Jäckle H, Gruss P, Mansouri A. mBtd is required to maintain signaling during murine limb development. Genes and Development. 2003;17(21):2630–2635. [PubMed]
112. Waclaw RR, Allen ZJ, II, Bell SM, et al. The zinc finger transcription factor Sp8 regulates the generation and diversity of olfactory bulb interneurons. Neuron. 2006;49(4):503–516. [PubMed]
113. Ala U, Piro RM, Grassi E, et al. Prediction of human disease genes by human-mouse conserved coexpression analysis. PLoS Computational Biology. 2008;4(3) Article ID e1000043. [PMC free article] [PubMed]
114. Pellegrino M, Provero P, Silengo L, Di Cunto F. CLOE: identification of putative functional relationships among genes by comparison of expression profiles between two species. BMC Bioinformatics. 2004;5 Article ID e1000043. [PMC free article] [PubMed]
115. Candi E, Terrinoni A, Rufini A, et al. p63 is upstream of IKKα in epidermal development. Journal of Cell Science. 2006;119(22):4617–4622. [PubMed]
116. Lewandoski M, Sun X, Martin GR. Fgf8 signalling from the AER is essential for normal limb development. Nature Genetics. 2000;26(4):460–463. [PubMed]
117. Moon AM, Capecchi MR. Fgf8 is required for outgrowth and patterning of the limbs. Nature Genetics. 2000;26(4):455–459. [PMC free article] [PubMed]
118. Han J, Ishii M, Bringas P, Jr., Maas RL, Maxson RE, Jr., Chai Y. Concerted action of Msx1 and Msx2 in regulating cranial neural crest cell differentiation during frontal bone development. Mechanisms of Development. 2007;124(9-10):729–745. [PMC free article] [PubMed]
119. Cobb J, Duboule D. Comparative analysis of genes downstream of the Hoxd cluster in developing digits and external genitalia. Development. 2005;132(13):3055–3067. [PubMed]
120. Vieux-Rochas M, Mantero S, Heude E, et al. Spatio-temporal dynamics of gene expression of the Edn1-Dlx5/6 pathway during development of the lower jaw. Genesis. 2010;48(6):362–373. [PubMed]
121. Panganiban G, Rubenstein JLR. Developmental functions of the Distal-less/Dlx homeobox genes. Development. 2002;129(19):4371–4386. [PubMed]
122. Depew MJ, Simpson CA, Morasso M, Rubenstein JLR. Reassessing the Dlx code: the genetic regulation of branchial arch skeletal pattern and development. Journal of Anatomy. 2005;207(5):501–561. [PubMed]
123. Lu P, Minowada G, Martin GR. Increasing Fgf4 expression in the mouse limb bud causes polysyndactyly and rescues the skeletal defects that result from loss of Fgf8 function. Development. 2006;133(1):33–42. [PubMed]
124. Costanzo AD, Festa L, Roscigno G, et al. A dominant mutation etiologic for human tricho-dento-osseous syndrome impairs the ability of DLX3 to downregulate ΔNp63α Journal of Cellular Physiology. 2011;226(8):2189–2197. [PubMed]
125. Paina S, Garzotto D, DeMarchis S, et al. Wnt5a is a transcriptional target of Dlx homeogenes and promotes differentiation of interneuron progenitors in vitro and in vivo. Journal of Neuroscience. 2011;31(7):2675–2687. [PubMed]
126. Yamaguchi TP, Bradley A, McMahon AP, Jones S. A Wnt5a pathway underlies outgrowth of multiple structures in the vertebrate embryo. Development. 1999;126(6):1211–1223. [PubMed]
127. Eisenberg LM, Ingham PW, Brown AMC. Cloning and characterization of a novel Drosophila Wnt gene, Dwnt-5, a putative downstream target of the homeobox gene distal-less. Developmental Biology. 1992;154(1):73–83. [PubMed]
128. Topol L, Jiang X, Choi H, Garrett-Beal L, Carolan PJ, Yang Y. Wnt-5a inhibits the canonical Wnt pathway by promoting GSK-3-independent β-catenin degradation. Journal of Cell Biology. 2003;162(5):899–908. [PMC free article] [PubMed]
129. Barrow JR, Thomas KR, Boussadia-Zahui O, et al. Ectodermal Wnt3β-catenin signaling is required for the establishment and maintenance of the apical ectodermal ridge. Genes and Development. 2003;17(3):394–409. [PubMed]
130. Church VL, Francis-West P. Wnt signalling during limb development. International Journal of Developmental Biology. 2002;46(7):927–936. [PubMed]
131. Geetha-Loganathan P, Nimmagadda S, Scaal M. Wnt signaling in limb organogenesis. Organogenesis. 2008;4(2):109–115. [PMC free article] [PubMed]
132. Yang Y. Wnts and Wing: Wnt signaling in vertebrate limb development and musculoskeletal morphogenesis. Birth Defects Research Part C. 2003;69(4):305–317. [PubMed]
133. Barton C, Johnson K, Mays D, et al. Novel p63 target genes involved in paracrine signaling and keratinocyte differentiation. Cell Death and Disease. 2010;1, article e74 [PMC free article] [PubMed]
134. Shalom-Feuerstein R, Lena AM, Zhou H, et al. ΔNp63 is an ectodermal gatekeeper of epidermal morphogenesis. Cell Death and Differentiation. 2011;18:887–896. [PMC free article] [PubMed]

Articles from Journal of Biomedicine and Biotechnology are provided here courtesy of Hindawi