Mutations in human Exostosin genes (EXTs) confer a disease called Hereditary Multiple Exostoses (HME) that affects 1 in 50,000 among the general population. Patients with HME have a short stature and develop osteochondromas during childhood. Here we show that two zebrafish mutants, dackel (dak) and pinscher (pic), have cartilage defects that strongly resemble those seen in HME patients. We have previously determined that dak encodes zebrafish Ext2. Positional cloning of pic reveals that it encodes a sulphate transporter required for sulphation of glycans (Papst1). We show that although both dak and pic are required during cartilage morphogenesis, they are dispensable for chondrocyte and perichondral cell differentiation. They are also required for hypertrophic chondrocyte differentiation and osteoblast differentiation. Transplantation analysis indicates that dak−/− cells are usually rescued by neighbouring wild-type chondrocytes. In contrast, pic−/− chondrocytes always act autonomously and can disrupt the morphology of neighbouring wild-type cells. These findings lead to the development of a new model to explain the aetiology of HME.
Hereditary Multiple Exostoses is a disease that causes the formation of benign bone tumours in children. Besides causing severe skeletal deformity, the bone tumours can compress nerves or other tissue resulting in chronic pain. Although the tumours can usually be surgically removed, they sometimes recur or are in positions that prevent surgery. We have identified two strains of zebrafish whose offspring have skeletal defects that resemble those of patients with Hereditary Multiple Exostoses. We have found that each strain carries a mutated form of an essential gene. Importantly, these two genes are also found in humans, and thus by analysing their function in zebrafish, we may shed light on their role in humans. Our study has elucidated the roles of these genes during normal skeletal development and has allowed us to generate a model for how genetic changes give rise to bone tumours in humans.
Citation: Clément A, Wiweger M, von der Hardt S, Rusch MA, Selleck SB, Chien C-B, et al. (2008) Regulation of Zebrafish Skeletogenesis by ext2/dackel and papst1/pinscher. PLoS Genet 4(7): e1000136. doi:10.1371/journal.pgen.1000136
Editor: Mary Mullins, University of Pennsylvania School of Medicine, United States of America
Received: January 30, 2008; Accepted: June 20, 2008; Published: July 25, 2008
Copyright: © 2008 Clément et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by grants from Cancer Research UK (C11413), the Wellcome Trust (072346/Z/03/Z) and the European Commission (LSHM-CT-2003-504468) to HHR and an HFSP grant (RGP0044/2006-C) to CBC. The MRC Centre for Developmental and Biomedical Genetics is supported by Grant G070091.
Competing interests: The authors have declared that no competing interests exist.
Mutations in human EXT1 and EXT2 confer an autosomal dominant disorder called HME ,,. Both EXT1 and EXT2 encode glycosyltransferases that together form a hetero-oligomeric complex in the Golgi and catalyse the polymerisation of sugars to form heparan sulphate (HS) (for review see ). Patients with HME have a short stature and during childhood develop osteochondromas (also called cartilaginous exostoses) that first appear near the growth plate regions of their skeleton. Osteochondromas are made up of a cartilage cap that resembles a growth plate and a bony collar that forms a marrow cavity that is contiguous with the underlying bone. While osteochondromas are normally benign, they can lead to complications and patients have a 1–2% risk of developing chondrosarcoma or osteosarcoma. Most of the tested patients with HME are heterozygous for mutations in either EXT1 (41%) or EXT2 (30%) –. Determining the genetic basis for the cases that cannot be attributed to EXT genes (29%) is essential for counselling HME patients.
The sporadic and dominant nature of osteochondromas formation in HME patients has led to the proposal of two genetic models (For discussion see ). Osteochondromas may arise from a loss-of-heterozygosity (LOH) at one of the EXT loci in skeletal cell resulting in unregulated growth and clonal expansion. In support of this model, LOH due to somatic mutations or aneuploidy has been identified in a small number of the osteochondromas analysed ,. In addition, HS is absent in chondrocytes within osteochondromas which is consistent with a complete loss of EXT function due to LOH . Contrary to this model, HS is secreted and it is likely that a homozygous mutant chondrocyte would be rescued by contact with neighbouring cells. The alternative model is that reduced EXT gene dosage causes reduced HS synthesis that results in a structural change in the growth plate. This change allows chondrocytes to occasionally escape normal developmental constraints to give rise to an osteochondroma. The finding that the majority of analysed exostoses do not show a second mutation in the EXT gene family lends support to the gene dosage theory . Resolving between these two models could play an important role in designing future treatment for HME patients.
Skeletal histology in fish is comparable to that of tetrapods  and the development of the cranial skeleton of zebrafish has been well described ,. The precartilage condensations that will give rise to the cartilaginous skeleton begin to appear during the second day of development. Condensations give rise to two cell types: the cells of the perichondrium (a sheath that encapsulates the cartilage) and the chondrocytes that begin to secrete the cartilage matrix. As the skeleton forms, some chondrocytes flatten and intercalate to form a column that gives rise to rod shaped cartilage elements. Alternatively, chondrocytes flatten to form a single layer of tessellated cells that give rise to plate-like elements . Much of the cartilaginous skeleton is then replaced by bone in a process that resembles endochondral ossification in tetrapods. These bones are referred to as cartilage bones. Also, like tetrapods, some of the bony skeleton does not form from a cartilage template. These bones are called intramembranous (or dermal) bones.
Large-scale genetic screens have identified many genes that disrupt skeletal development in zebrafish –. Here we have focused on two genes that are required for skeletal development, dak and pic. Both dak and pic, along with a third gene boxer, are also required for fin development , and axon sorting  suggesting that the mutated genes act in a common pathway. We have previously shown that dak and boxer encode glycosyltransferases required for HS synthesis (ext2/dak, extl3/boxer) . In this study we present evidence that pic encodes a putative PAPS transporter (3′-phosphoadenosine 5′-phosphosulfate transporter, PAPST1) that is required for sulphation of glycans. We show that dak and pic are required for cartilage morphogenesis, but surprisingly not for early cartilage differentiation. We show that hypertrophic differentiation of chondrocytes and subsequent cartilage bone formation is lost in mutant larvae. We also show that intramembranous bone formation is reduced due to a reduction of osteoblast differentiation. We show that dak and pic can act cell autonomously during chondrogenesis, and based upon these findings propose a model for how LOH could account for osteochondroma formation in HME patients.
Chondrocyte Morphology dak−/− and pic−/− Larvae Resembles that Found in HME Patients
Chondrocytes in osteochondromas often differ from chondrocytes found in normal growthplates. Instead of being flattened and forming long columns of cells, they are usually rounded and form clusters of cells ,,. We wondered whether chondrocytes in dak−/− and pic−/− mutants behave in a similar way. Although most of the cartilage elements are present in both dak−/− and pic−/− larvae, the elements are shorter and thicker than wild-type (Figure 1A,D,G) . In dak−/− larvae, anterior cartilages tend to have more cells than wild-type and posterior cartilages have less. For example, in 144hpf dak−/− larvae the Meckel's cartilage much larger than in wild-type, while ceratobranchial 4 is small or even absent (H.R. and M.W. unpublished). Wild-type chondrocytes flatten along the longitudinal axis (stack) in most elements (Figure 1A–C) and in rod shaped elements the cells intercalate to form a single column (Figure 1B). Some elements have regions where stacking is not obvious (arrowhead in Figure 1C) especially in regions adjacent to joints (arrowheads in Figure 1B). In all dak−/− larvae, all chondrocytes are round and do not form into columns (Figure 1D–F). While pic−/− larvae show lower expressivity, most larvae have a loss of chondrocyte organisation that resembles that seen in dak−/− larvae (Figure 1G–I). One striking difference between dak−/− and pic−/− larvae is that pic−/− larvae do not stain with Alcian Blue at pH1.0 (Figure 1D,G) but do stain at pH2.5 (M.W. and A.C. unpublished).
Skeletal preparations of wild-type (A–C), dak−/− (D–F) and pic−/− (G–I) at day 6 reveal the shape of the cartilaginous skeleton as well as chondrocyte morphology. Ventral views of the head show that the cartilage elements of dak−/− and pic−/− fish are shorter and thicker than wild-type (A,D,G). Dissected cartilage laid flat show a complete lack of chondrocyte flattening and intercalation in skeletal elements from dak−/− and pic−/− larvae (B,E,H ceratobranchial 1; C,F,I hyosymplectic). Arrowheads in B and C indicate regions that lack stacking in wild-type embryos. Alcian Blue staining at pH1.0 (HCl 0.1N) does not stain pic−/− cartilage (G,H,I). Camera lucida drawings of chondrocytes in wild-type and mutant larvae (B',E',H'). Scale bars = 50μM.
Sulphate Synthesis Is Affected in pic−/− Embryos
As Alcian Blue preferentially stains sulphated groups at low pH , one possible explanation for the lack of staining in pic−/− larvae is a loss of sulphation of glycans and other sulphated moieties. To investigate this further, we used antibodies for HS , CS  and KS  and found that whereas HS is reduced in both dak−/− and pic−/− larvae (Figure 2A–C), CS and KS are reduced only in pic−/− larvae (Figure 2D–I). The antibody used to detect heparin, 10E4, recognizes an epitope that is localised to basal laminae, but not found in the developing zebrafish cartilage (Figure S2). We further analysed HS composition using heparan lyase digestion followed by HPLC . Peaks generated by zebrafish larval extracts were compared to 6 known standards. pic−/− embryos show a severe reduction of sulphated disaccharides, but surprisingly also show a reduction in unsulphated disaccharides (Figure 2J). This perhaps indicates that the loss of sulphation affects processing or stability of heparan. However, it is important to note that in the absence of sulphation, heparan synthesis may generate atypical disaccharides which would not be identified by this analysis . Together these data confirm that pic is required for sulphation of proteoglycans.
Whole mount antibody staining at 24hpf reveals that HS is reduced in the somites of dak−/− and pic−/− (A–C) and KS in the notochord is reduced only in pic−/− larvae (D–F). Cartilage staining of the ceratohyal at 72hpf reveals that CS is made in wild-type and dak−/− chondrocytes (red stain in G,H), and absent from pic−/− cartilage (I) (nuclear staining is shown in blue with DAPI). HPLC analysis of HS in pic−/− larvae at day 5 indicates that sulphated disaccharides are nearly absent and unsulphated disaccharides are reduced (red) compared to their siblings (blue) (J). 1: ΔUA-GlcNAc, unsulfated Δ4,5-unsaturated hexuronate -N-acetyl glucosamine; 2: ΔUA-GlcNS, ΔUA-N-sulfated glucosamine; 3: ΔUA-GlcNAc6S, ΔUA-6-O-sulfated GlcNAc; 4: ΔUA-GlcNS6S, ΔUA-N-sulfated, 6-O-sulfated glucosamine; 5: ΔUA2S-GlcNS, 2-O-sulfated ΔUA-N-sulfated glucosamine; 6: ΔUA2S-GlcNS6S, 2-O-sulfated ΔUA-N-sulfated, 6-O-sulfated glucosamine. These disaccharides correspond to the major disaccharides found in both invertebrate and vertebrate animals. Panel F scale bar = 50μM. Panel I scale bar = 10μM.
pic Encodes a PAPST1, a New Candidate Gene for HME
29% of patients with HME do not carry mutations in EXT1 or EXT2 genes. In order to help identify new candidate genes, we positionally cloned pic. Using SSLP microsatellite markers, we mapped the pic locus to a 3.3cM interval on chromosome 20 (Figure 3A). Using the zebrafish RH map, we placed a zebrafish gene with homology to human and Drosophila PAPST1 , in the same interval (Figure 3C and Table S1). As PAPST1 transports PAPS into the Golgi (PAPS being the universal donor for sulphation), it is a good candidate gene to explain the loss of proteoglycan sulphation. We then sequenced papst1 cDNA from picto216z/to216z and picto14mx/to14mx mutant embryos (Figure 3B). The picto216z allele has a nucleotide transition (G to A) at position 390 in the third exon, creating a stop codon. The picto14mx allele is a genomic deletion that results in an in-frame deletion of all of exon 3 in the cDNA. To confirm that mutations in papst1 result in the pic−/− phenotype, we expressed the wild-type zebrafish papst1 cDNA under the control of a heterologous promoter in pic−/− embryos. Expression of wild-type papst1 in a single cell was sufficient to rescue staining of KS in the notochord (Figure 3D–F). To determine the expression pattern of papst1, we performed wholemount in situ hybridization with the full-length cDNA. Consistent with its role as a general component of the cellular sulphation machinery, papst1 is expressed ubiquitously (Figure S1). As both alleles are predicted to result in severe truncation of the PAPST1 protein and have identical phenotypes, they are likely to be null alleles.
Genetic map of pic locus (A). Note that z1534 has not been assigned a genetic position as it was found on the RH map. Allele sequencing identifies picto216z as a premature stop codon in exon 3 and picto14mx as a deletion of exon 3 (B). Zebrafish PAPST1 clusters with human and Drosophila PAPST1 in a dendrogram (C). Expression of wild-type PAPST1 in a single notochord cell rescues synthesis of KS in pic−/− larvae (D–E). Close-up of single cell secreting KS in brown (arrow in E), and the same cell counterstained for the rescue construct reporter in purple (arrow in F). The dendrogram was made using Clustal W and Treeview68k. Accession numbers: AB107958, NP_648954, AB106538, NP_057032, NP_991198, NP_001035084, NM_005827. Zebrafish and human PAPST1 share 70% amino acid identity. Panel D scale bar = 100μM. Panel E scale bar = 50μM.
The Onset of Cartilage Differentiation Is Normal in dak−/− and pic−/− Larvae
The LOH model for HME raises the question of whether EXT−/− cells could differentiate into all the cell types that make up an osteochondroma. To address this question, we first tested whether perichondral cells and chondrocytes differentiate normally in dak−/− and pic−/− mutant larvae. Surprisingly, expression of three markers of early chondrogenesis occurs in both mutants as in wild-type larvae (Figure 4A–I). To test whether the perichondrium is present, we used a marker, gdf5, which is expressed in the perichondrium of the ceratohyal . Expression is present in the ceratohyal of both mutants (arrows in Figure 4J–L). The flattened cells of the perichondrium can also be seen in toluidine blue stained sections of mutant larvae, indicating that HS is dispensable for the differentiation and morphogenesis of these cells (arrows in Figure 4M–O). Together, these data suggest that the cartilage and perichondral components of osteochondromas could be formed by EXT−/− cells.
Wholemount RNA in situ analysis of sox9a (A–C), collagen2a1a (D–F), chondromodulin (G–I) and gdf5 (J–L) at 60hpf (all ventral views of the head). Although the position of the developing skeleton varies between wild-type and mutants, the markers are expressed at similar levels in wild-type (A,D,G,J), dak−/− (B,E,H,K) and pic−/− (C,F,I,L). dak−/− larvae express sox9a at higher levels anteriorly, but this is perhaps due to more chondrogenic cells being present (see Figure 6). Expression of gdf5 in the perichondrium of the ceratohyal is present albeit slightly reduced in dak−/− and pic−/− (arrows in J–L). The perichondrium of the hyosymplectic is also seen in toluidine blue stained sections at day 5 (arrows in M,N,O). Panel I scale bar = 50μM. Panel L scale bar = 5μM.
Ossification Is Reduced in both dak−/− and pic−/− Larvae
As osteochondromas contain a bony collar, we next tested whether bone forms normally in homozygous dak−/− and pic−/− larvae. Intramembranous (dermal) and cartilage bones appear during early larval development . Alizarin Red staining for bone at 144hpf shows a strong reduction of calcification in both bone types (Figure 5J–L). Consistent with this, there is a strong reduction of several markers for osteoblast differentiation in both mutants at 96hpf (Figure 5A–I and see Table S2). As cartilage hypertrophy precedes endochondral ossification, we also tested whether expression of the hypertrophic marker, collagen10a1 is affected at 144hpf. We found that chondrocyte expression of collagen10a1 is absent in both mutants (arrows in Figure 5 M–O). Together these data suggest that EXT−/− cells in an osteochondroma would not contribute significantly to the formation or remodelling of bone. Thus it is likely that EXT−/+ cells would be recruited to an osteochondroma and take part in the formation of the bony collar.
Wholemount RNA in situ analysis of osterix (A–C), crossveinless (D–F) and collagen10a1 (G–I) at 96hpf (all ventral views of the head). Markers for dermal and cartilage bone development are down-regulated or absent in both mutants (A,D,G wild-type; B,E,H dak−/−; C,F,I pic−/−). Arrows indicate wild-type expression in the maxilla (A), branchiostegal ray (D) and opercle (G). The loss of marker gene expression is consistent with the later reduction in bone formation in ventral views of 6 day old larvae stained with Alizarin Red (J,K,L). Arrows indicates the location of the cleithrum in J, K and L. Table S2 lists all of the affected bones. collagen10a1 expression in chondrocytes of the ceratohyal in wild-type larvae marks chondrocytes as they become hypertrophic (arrow in M). This expression is absent in dak−/− (N) and pic−/− (O) larvae. Panel L scale bar = 100μM. Panel O scale bar = 10μM.
Pre-Cartilage Condensations form but Chondrocyte Cell Behaviour Is Deficient in dak−/− Embryos
To determine when chondrocyte behaviour is first affected in dak−/− embryos, we looked at condensation formation in the jaw. Early condensations within the first arch were visualized at 45 and 50hpf using sox9a as a chondrogenic marker (Figure 6A–D). Even at this early stage, dak−/− chondrocytes appeared more round than those in wild-type embryos (as judged by nuclear morphology, arrows in Figure 6C,D). In anterior condensations, the level of sox9a expression is variable and usually stronger in dak−/− condensations, consistent with the increase in chondrocyte cell number seen in anterior arches (Figure 6B,D). We also examined early stacking within condensations of the second arch at 54 and 58hpf. During this time wild-type chondrocytes intercalated to form a single cell layer, flattened perpendicular to the growth axis and began to secrete cartilage matrix (Figure 6E,E',G,G'). Although dak−/− chondrocytes also began secreting matrix, the cells showed no signs of undergoing morphogenesis (Figure 6F,F',H,H'). Taken together, these data suggest that the primary cartilage defect in dak−/− larvae is the loss of chondrocyte organisation. Similar results were obtained with pic−/− larvae but with lower and more variable expressivity (data not shown).
Pre-cartilage condensations in the first arch are larger in dak−/− larvae as judged by sox9a staining at 45hpf (A,B) and 50hpf (C,D). Individual cells within the condensation appear to have a more rounded morphology in dak−/− larvae than in wild-type larvae (compare arrows in C,D). Intercalation and flattening of chondrocytes to give rise to the ceratohyal cartilage in the second arch takes place between 54 and 58hpf in wild-type (E,G), but does not occur in dak−/− larvae (F,H). Chondrocytes begin to secrete cartilage matrix during this time as seen by Alcian Blue staining (G,H). Camera lucida drawings of chondrocytes in wild-type and dak−/− larvae (E'–H'). Scale bars = 10μM.
dak−/− Chondrocytes Show both Autonomous and Non-Autonomous Behaviour
One caveat in the LOH model is that HS is secreted and thus an EXT−/− cell that arises would be rescued by neighbouring cells. To ascertain whether clones of dak−/− cells behave autonomously when juxtaposed to HS secreting cells, we transplanted dak−/− cells into wild-type embryos. The transplantations were done at sphere stage, then the embryos were allowed to develop for several days before fixation and analysis. We found that in most cases (19/24 transplants), the transplanted mutant cells stacked normally when juxtaposed to wild-type cells (arrow, Figure 7B). This alone would argue that single EXT−/−cells in HME patients would be unable to form exostoses and thus would refute the LOH model. However in some cases (5/24) mutant cells behaved autonomously and failed to stack or intercalate (arrowheads, Figure 7C–E). These mutant clones grew out from the edge of the cartilage perpendicular to the wild-type stacks. Given that HS may not diffuse far, it is plausible that dak−/− cells on the edge of the cartilage lack sufficient contact to be rescued by neighbouring wild-type chondrocytes. This explanation is consistent with studies of HME patients that have found that osteochondromas are first seen on the edge of the growth plate just beneath the perichondrium ,. Importantly, this results shows that cells that ext2−/− chondrocytes can behave autonomously in zebrafish and thus EXT−/− chondrocytes in humans could be responsible for the formation of osteochondromas.
Transplanted dak−/− cells usually form columns with wild-type chondrocytes (arrow in B). However, in some cases dak−/− cells grow out from the wild-type host cells and behave autonomously (arrowheads in C,D,E). pic−/− cells transplanted into wild-type hosts never stack (arrowheads in F,G). In addition, wild-type cells both stack (arrows in H,I) and fail to stack (arrowheads in H,I) when transplanted into pic−/− hosts. Wild-type cells that stack in pic−/− hosts form columns that lie parallel to the longitudinal axis (grey arrow in I). (A–I) Dissected cartilage elements; all are ceratobrachial cartilage except (E) and (I) which are trabecular and ceratohyal cartilage respectively. Brown cells in (A–G) are transplanted cells, blue cells in (H,I) are transplanted cells. (J) summarises all 63 transplants analysed. Transplanted cells that flattened also intercalated to form columns. WT = wild-type.
pic−/− Chondrocytes Have Autonomous Behaviour
In all transplants examined (39/39), pic−/− cells behaved autonomously and failed to stack or intercalate (arrowheads, Figure 7F,G). In addition, when juxtaposed to pic−/− cells, wild-type cells often adopted the mutant rounded morphology (arrowheads, Figure 7H,I). In many cartilage elements, both stacked and non-stacked clusters of wild-type chondrocytes were seen (20/39). Significantly, whenever wild-type cells stacked, they flattened and formed columns that were oriented to the longitudinal axis of the cartilage element, even when few wild-type cells were present in a pic−/− cartilage element (arrow, Figure 7I). This suggests that there is a signal that polarizes chondrocytes so that stacking is oriented to the correct axis and that this signal is still present in pic−/− larvae. These findings are also consistent with the LOH model and suggest that patients with mutations in PAPST1 may have more severe clinical symptoms.
The LOH Model for Osteochondroma Formation
While much is known about the genetic basis of HME, the mechanism of osteochondroma formation is poorly understood. In this study, we show that zebrafish is an excellent model for HME and our findings support the LOH model in several ways. First, proliferating chondrocytes in osteochondromas resemble those seen in homozygous dak−/− larvae: they are rounded and do not form into columns of cells ,,. Second, we show that homozygous mutant cells differentiate into chondrocytes, despite the absence of morphogenesis. Third, transplants with dak−/− cells into wildtype animals show that although most homozygous mutant clones were rescued, some dak−/− chondrocytes behaved autonomously. The rescue of mutant cells is presumably due to HS secretion from neighbouring wild-type cells, but may also be due to other secreted factors. The results presented here as well as from other studies suggest a model for how LOH could result in osteochondroma formation (Figure 8). Although our results lend credence to the LOH model, they do not refute the gene dosage model and it is possible that both mechanisms play a role.
(A) EXT−/− chondrocytes that originate or end up on the edge of the growth plate lose the ability to respond to a polarity signal. These chondrocytes adopt a round morphology and do not contribute to the neighbouring columns of chondrocytes. The LOH may occur during early skeletal development, before formation of the bony collar. (B) As EXT−/− chondrocytes proliferate they form a clone of cells that begin to grow out from skeleton beneath the EXT−/+ perichondrium. (C) EXT−/+ chondrocytes join the clone of EXT−/− cells, express collagen10 and become hypertrophic. EXT−/+osteoblasts are recruited to form the bony collar. This results in the cartilage cap being predominantly composed of EXT−/− chondrocytes, while the cells that make up the rest of the osteochondroma (hypertrophic chondrocytes, osteoblasts and perichondrial cells) are predominantly EXT−/+.
Different Phenotypes in Mouse and Zebrafish Models for HME
Several studies of the role of EXT genes during mouse skeletogenesis have been published and these favour the gene dosage model for HME. In mice homozygous for a hypomorphic allele of Ext1 (Ext1gt/gt) or heterozygous for a targeted deletion (Ext1+/−), the chondrocytes of limb growth plates show delayed hypertrophic differentiation and endochondral ossification ,. Given that HS is known to regulate the activity of many signalling pathways, the researchers tested whether a signalling defect could explain the Ext1 mutant phenotype. Indian Hedgehog (IHH), a signalling protein that normally acts in the growth plate to block hypertrophy and terminal differentiation of chondrocytes was found to have increased activity in mutant mice. The model for these results is that in wild-type animals, HS normally acts to limit diffusion of IHH and thereby allow chondrocytes to become hypertrophic ,. The authors favour the gene dosage model for HME and propose that hereditary osteochondromas are caused in part by a delay in chondrocyte hypertrophy caused by excessive IHH signalling ,. In contrast, mice heterozygous for a targeted deletion of Ext2 (Ext2+/−) have normal limb growth plates and there is no discernible effect on IHH diffusion . However, Ext2+/− mice do have osteochondroma-like outgrowths on their ribs. These authors also favour the gene dosage model but do not find evidence to support a role for IHH.
In comparison, dak−/− and pic−/− larvae show a more severe skeletal phenotype, perhaps due to a stronger reduction of HS. Whereas mice homozygous for null mutations in Ext1 or Ext2 in mice arrest during gastrulation ,, dak−/− and pic−/− embryos can gastrulate probably due to maternally deposited RNAs ( and Figure S1). By 36hpf, HS is only weakly detectable in dak−/− and pic−/− embryos (by immunohistochemistry, AC and MW unp). The early reduction of HS has enabled us to identify cartilage morphogenesis as the primary defect during skeletogenesis. Indeed, chondrocytes in both Ext1gt/gt and Ext2+/− mice show a mild disruption of the columnar organization within the growth plate ,. Thus it is likely that complete loss of stacking, as early as the cartilage condensation phase, would be evident with a more severe reduction of mouse Ext gene function.
IHH signalling is not likely to be responsible for the cartilage morphogenesis phenotype because neither of the two zebrafish IHH genes is expressed until 2 days after chondrocyte stacking begins. Furthermore, pharmacological inhibition of Hedgehog signalling during skeletogenesis does not affect chondrocyte stacking (MW and AC unpublished). One plausible candidate for this signal in zebrafish is wnt5b which encodes a ligand for the non-canonical WNT signalling pathway . The evidence for this is that wnt5b is expressed in cells surrounding cartilage condensations and mutations in wnt5b result in reduced chondrocyte stacking (MW and AC unpublished). As the wnt5b−/− cartilage phenotype is mild compared to that of dak−/− larvae, other members of the non-canonical WNT family of genes may be redundant with wnt5b. An intriguing possibility is that WNT signalling and other components of the planar cell polarity system mediate chondrocyte stacking, just as they regulate convergence/extension movements during gastrulation.
Although early chondrocyte differentiation is unaffected in zebrafish mutant larvae, we did find that expression of the hypertrophic marker, collagen10a1, is lost. This is in agreement with results from Ext1 mutant mice which show a delay in chondrocyte hypertrophy due to increased IHH signalling ,. The opposite result has been found for Ext2 mutant mice where a reduction in HS was shown to cause premature collagen10 expression . Intriguingly, studies of HME patients have found evidence of premature hypertrophy in osteochondromas ,. Determining why apparently conflicting results have been obtained in these systems will require more detailed analysis.
HS has been implicated in osteoblastogenesis, however there has been no clear evidence for a developmental role to date . Here we show that osteoblastogenesis is impaired by the reduction of HS mutant zebrafish larvae. Although previous Ext mutant mouse studies have focused on cartilage differentiation, a reduction in the bone mineral density of Ext1+/− mice has been observed . Furthermore, osteopenia has been shown to be associated with HME in a family that carries a mutation in EXT1 . These findings suggest a new role for HS during osteoblast differentiation.
PAPST1 as a Candidate Gene for HME
While most of the tested patients with HME are heterozygous for mutations in either EXT1(41%) or EXT2 (30%), the genetic basis of the remaining cases is unknown (29%) –. Several EXT-like genes have been shown encode enzymes required during HS synthesis and would thus make good candidate genes (EXTL1, EXTL2, and EXTL3). Unfortunately, none of these have been shown to carry disease-related mutations in HME patients . Although mutations in sulphate metabolism can cause hereditary skeletal disorders, none of these results in the formation of osteochondromas –. Here we show for the first time that PAPST1 is essential for sulphation of glycans in vertebrates and that mutations in pic confer a specific phenotype that is very similar to the dak−/− phenotype. This is a surprising result because unlike dak mutations which only reduce HS, pic mutations should reduce all sulphation in the cell. Inactivation of PAPST genes in Drosophila also results in phenotypes that resemble EXT mutant phenotypes ,. Together, these findings suggest that although other glycans may be required during vertebrate and invertebrate development, HS is the principal glycan. Furthermore, our results suggest that PAPST1 as well as other genes involved with sulphate transport and metabolism are candidate genes for HME.
Materials and Methods
Unless otherwise stated, all methods were based upon standardised protocols . For dak mutant analysis, allele to273b was used for all analysis, as it should result in a complete loss of Ext2 function . dak−/− larvae were identified by the absence of fins. For pic analysis, allele to14mx was used unless otherwise stated. To identify pic−/− larvae before the phenotype is morphologically visible, genomic DNA was extracted, and PCR was performed using TAQ polymerase and the following primers: F2: 5′CGT GTG ATG ACG CGC TCA TAC 3′
R1ab: 5′AGC GCC AGG ATG CGG TTC AT 3. The conditions were 94°C (30 seconds), 55°C (60 seconds) and 72°C (60 seconds) for 35 cycles. DNA from homozygous mutants does not generate a band as the 14mx mutation deletes this region.
Genetic Mapping and Cloning of pic
The pic locus was mapped to linkage group 20 (lg20) after analysing SSLP (simple sequence length polymorphism) markers on 700 meioses. picto14mx maps 2.7cM south of z1534 (20/740 meiosis) and 0.6cM north of z8554 (4/698 meiosis) . This interval on the T51 radiation hybrid (RH) map  was found to contain many ESTs. A contig in the neighborhood of one of these, fc88f04.x1, was assembled using traces from the Sanger Centre, and found to contain a gene having homology to a human and Drosophila PAPS Transporter 1 (PAPST1, also known as: Solute Carrier Family 35, Member B2) ,. To confirm the location of zebrafish papst1, primers were designed to exon 4 and analysed using the T51 panel (papstf3, 5′ CGTCACCACATTCTCCGGCGT 3′ and papstr3, 5′GTGTCTGATTTCCTGAAGTGT 3′). The papst1 pattern matches the pattern of other markers in the pic interval (see Table S1). To sequence alleles, cDNA was obtained from picto14mx/to14mx, picto216z/to216z larvae and wild-type larvae and then sequenced with primers papstf1 and papstf1.1e (respectively, 5′ TGGCAGTTTTGTAGAGGCGGAG 3′ and 5′ GAATGCAGACGCTGTAGAC 3′).
Wholemount Antibody and mRNA in situ Staining
Primary antibodies were anti-HS 1∶500 (10E4, Europa), anti-keratan sulphate 1∶100 (KS) (3H1, Developmental Studies Hybridoma Bank), anti-chondroitin sulphate 1∶100 (CS) (CS-56, Sigma), anti-collagen type II 1∶200 (II-II6B3, Developmental Studies Hybridoma Bank) and anti-GFP 1∶100 (Torrey Pines Biolabs). Secondary antibodies were horse anti-mouse-HRP and goat anti-rabbit-HRP (Vector Laboratories). Detection was done using DAB substrate (Vector Laboratories) or TSA-CY3 substrate (Perkin Elmer). Larvae were mounted in 70% glycerol or Vectashield with DAPI (Vector). Antisense probes were made using the following cDNAs: chondromodulin1 , collagen2a1a , collagen10a1 , growth and differentiation factor-5 (gdf5/contact) , crossveinless2  and sox9a . Cloning and characterisation of zebrafish osterix will be described elsewhere. Goat anti-DIG fab fragments and NBT/BCIP substrate (Roche) were used to develop the in situs.
Rescue of Keratan Sulphate Synthesis in pic−/− embryos
To rescue pic−/− embryos, we made an expression construct by cloning the wild-type zebrafish papst1 cDNA into an hspIG vector that contains a heat shock promoter and an IRES2 (internal ribosome entry site)/eGFP cassette (gift from Dr Florian Maderspacher). The construct was then injected into pic−/− larvae and the wild-type papst1 cDNA was expressed by heat shocking larvae at 24 hours post-fertilisation (hpf), for 1 hour at 38°C. The larvae were fixed 6 hours later and a double antibody staining was performed to check for rescue. As DNA injected at the one cell stage is inherited mosaically, the eGFP reporter was used to confirm that cells that synthesise keratan sulphate (KS) indeed carried the rescuing construct. First the larvae were stained using anti-KS with DAB as the substrate. After photographing, the embryos were then stained using anti-GFP with NBT/BCIP as the substrate to determine which cells carried the construct.
GFP donor embryos were first injected with tetramethyl-rhodamine dextran 3% (Invitrogen) at 1-cell stage. Then, both donors and recipients were dechorionated in pronase. Transplantation was done in E3 from sphere stage and based upon a zebrafish fate map (Woo and Fraser, 1995). At 24hpf, each recipient was screened for the presence of fluorescent rhodamine in the neural crest cells and kept until 120hpf with their donor. Larvae were then fixed in 4% PFA and Alcian Blue staining followed by antibody staining to track the GFP transplanted cells was performed. The experiment was done with picto216z/to216z or dakto273b/to273b transplanted into wild-type and vice versa.
papst1 is expressed ubiquitously. mRNA in situ analysis of papst1 expression: antisense (A–C) and sense (A prime–C prime) probes at the 30–60 cells stage (A, A prime), 50% epiboly stage (B, B prime) and 7 somites stage (C, C prime).
(1.51 MB EPS)
The 10E4 epitope is not expressed in the developing cartilage. Wildtype (A,C,E) and pic-/- (B,D,F) localisation of the 10E4 epitope (in green) at 60hpf. Cartilage (collagen type II) is shown in red and nuclei in blue (C–F). Side views of the whole fish (A,B), ventral views of the head (C,D) and high magnification pictures of the ceratohyal (E,F). The 10E4 epitope is detected predominantly on basal laminae but is undetectable in the developing cartilage at the time of chondrocyte stacking. Panel D scale bar = 100μM. Panel F scale bar = 10μM.
(9.71 MB EPS)
papst1 is physically linked to the pinscher genetic interval. PCR analysis of papst1 on the 94 hybrid cell lines from the T51 panel indicates that the majority of positive cell lines are also positive with SSLP markers that are genetically linked to pinscher.
(0.93 MB EPS)
Expression of bone markers as well as Alizarin Red staining is reduced in dak-/- and pic-/- larvae. Scoring was based upon larvae shown in Figure 5. An X indicates that expression is detectable, however expression was often reduced compared to wildtype.
(0.71 MB EPS)
We thank Chris Hill for assistance with histology, Robert Geisler for providing the RH panel and Torsten Trowe and Hans Georg Frohnhoefer for providing allele to14mx. The II-II6B3 antibody developed by T.F. Linsenmayer was obtained from the Developmental Studies Hybridoma Bank developed under the auspices of the NICHD and maintained by The University of Iowa, Department of Biological Sciences, Iowa City, IA 52242.
Conceived and designed the experiments: AC MW CBC HHR. Performed the experiments: AC MW SvdH MAR HHR. Analyzed the data: AC MW SvdH MAR SBS CBC HHR. Contributed reagents/materials/analysis tools: AC MAR SBS CBC HHR. Wrote the paper: AC MW HHR.
- 1. Zak BM, Crawford BE, Esko JD (2002) Hereditary multiple exostoses and heparan sulfate polymerization. Biochim Biophys Acta 1573: 346–355.
- 2. Ahn J, Ludecke HJ, Lindow S, Horton WA, Lee B, et al. (1995) Cloning of the putative tumour suppressor gene for hereditary multiple exostoses (EXT1). Nat Genet 11: 137–143.
- 3. Wuyts W, Van Hul W, Wauters J, Nemtsova M, Reyniers E, et al. (1996) Positional cloning of a gene involved in hereditary multiple exostoses. Hum Mol Genet 5: 1547–1557.
- 4. Duncan G, McCormick C, Tufaro F (2001) The link between heparan sulfate and hereditary bone disease: finding a function for the EXT family of putative tumor suppressor proteins. J Clin Invest 108: 511–516.
- 5. Alvarez C, Tredwell S, De Vera M, Hayden M (2006) The genotype-phenotype correlation of hereditary multiple exostoses. Clin Genet 70: 122–130.
- 6. Francannet C, Cohen-Tanugi A, Le Merrer M, Munnich A, Bonaventure J, et al. (2001) Genotype-phenotype correlation in hereditary multiple exostoses. J Med Genet 38: 430–434.
- 7. Xu L, Xia J, Jiang H, Zhou J, Li H, et al. (1999) Mutation analysis of hereditary multiple exostoses in the Chinese. Hum Genet 105: 45–50.
- 8. Porter DE, Simpson AH (1999) The neoplastic pathogenesis of solitary and multiple osteochondromas. J Pathol 188: 119–125.
- 9. Bovee JV, Cleton-Jansen AM, Wuyts W, Caethoven G, Taminiau AH, et al. (1999) EXT-mutation analysis and loss of heterozygosity in sporadic and hereditary osteochondromas and secondary chondrosarcomas. Am J Hum Genet 65: 689–698.
- 10. Hall CR, Cole WG, Haynes R, Hecht JT (2002) Reevaluation of a genetic model for the development of exostosis in hereditary multiple exostosis. Am J Med Genet 112: 1–5.
- 11. Hecht JT, Hall CR, Snuggs M, Hayes E, Haynes R, et al. (2002) Heparan sulfate abnormalities in exostosis growth plates. Bone 31: 199–204.
- 12. Huysseune A (2000) Skeletal System/Microscopic Functional Anatomy. In: Ostrander G,, editor. The Laboratory Fish. New York: Academic Press. pp. 307–317.
- 13. Cubbage CC, Mabee PM (1999) Development of the cranium and paired fins in the zebrafish Danio rerio (Ostariophysi, Cyprinidae). Journal of Morphology 229: 121–160.
- 14. Schilling TF, Kimmel CB (1997) Musculoskeletal patterning in the pharyngeal segments of the zebrafish embryo. Development 124: 2945–2960.
- 15. Kimmel CB, Miller CT, Kruze G, Ullmann B, BreMiller RA, et al. (1998) The shaping of pharyngeal cartilages during early development of the zebrafish. Dev Biol 203: 245–263.
- 16. Neuhauss SC, Solnica-Krezel L, Schier AF, Zwartkruis F, Stemple DL, et al. (1996) Mutations affecting craniofacial development in zebrafish. Development 123: 357–367.
- 17. Piotrowski T, Schilling TF, Brand M, Jiang YJ, Heisenberg CP, et al. (1996) Jaw and branchial arch mutants in zebrafish II: anterior arches and cartilage differentiation. Development 123: 345–356.
- 18. Schilling TF, Piotrowski T, Grandel H, Brand M, Heisenberg CP, et al. (1996) Jaw and branchial arch mutants in zebrafish I: branchial arches. Development 123: 329–344.
- 19. van Eeden FJ, Granato M, Schach U, Brand M, Furutani-Seiki M, et al. (1996) Genetic analysis of fin formation in the zebrafish, Danio rerio. Development 123: 255–262.
- 20. Norton WH, Ledin J, Grandel H, Neumann CJ (2005) HSPG synthesis by zebrafish Ext2 and Extl3 is required for Fgf10 signalling during limb development. Development 132: 4963–4973.
- 21. Trowe T, Klostermann S, Baier H, Granato M, Crawford AD, et al. (1996) Mutations disrupting the ordering and topographic mapping of axons in the retinotectal projection of the zebrafish, Danio rerio. Development 123: 439–450.
- 22. Lee JS, von der Hardt S, Rusch MA, Stringer SE, Stickney HL, et al. (2004) Axon sorting in the optic tract requires HSPG synthesis by ext2 (dackel) and extl3 (boxer). Neuron 44: 947–960.
- 23. Benoist-Lasselin C, de Margerie E, Gibbs L, Cormier S, Silve C, et al. (2006) Defective chondrocyte proliferation and differentiation in osteochondromas of MHE patients. Bone 39: 17–26.
- 24. Legeai-Mallet L, Rossi A, Benoist-Lasselin C, Piazza R, Mallet JF, et al. (2000) EXT 1 gene mutation induces chondrocyte cytoskeletal abnormalities and defective collagen expression in the exostoses. J Bone Miner Res 15: 1489–1500.
- 25. Lev R, Spicer SS (1964) Specific Staining of Sulphate Groups with Alcian Blue at Low Ph. J Histochem Cytochem 12: 309.
- 26. David G, Bai XM, Van der Schueren B, Cassiman JJ, Van den Berghe H (1992) Developmental changes in heparan sulfate expression: in situ detection with mAbs. J Cell Biol 119: 961–975.
- 27. Ito Y, Hikino M, Yajima Y, Mikami T, Sirko S, et al. (2005) Structural characterization of the epitopes of the monoclonal antibodies 473HD, CS-56, and MO-225 specific for chondroitin sulfate D-type using the oligosaccharide library. Glycobiology 15: 593–603.
- 28. Rauch U, Gao P, Janetzko A, Flaccus A, Hilgenberg L, et al. (1991) Isolation and characterization of developmentally regulated chondroitin sulfate and chondroitin/keratan sulfate proteoglycans of brain identified with monoclonal antibodies. J Biol Chem 266: 14785–14801.
- 29. Keller KM, Brauer PR, Keller JM (1989) Modulation of cell surface heparan sulfate structure by growth of cells in the presence of chlorate. Biochemistry 28: 8100–8107.
- 30. Kamiyama S, Suda T, Ueda R, Suzuki M, Okubo R, et al. (2003) Molecular cloning and identification of 3′-phosphoadenosine 5′-phosphosulfate transporter. J Biol Chem 278: 25958–25963.
- 31. Luders F, Segawa H, Stein D, Selva EM, Perrimon N, et al. (2003) Slalom encodes an adenosine 3′-phosphate 5′-phosphosulfate transporter essential for development in Drosophila. Embo J 22: 3635–3644.
- 32. Bruneau S, Mourrain P, Rosa FM (1997) Expression of contact, a new zebrafish DVR member, marks mesenchymal cell lineages in the developing pectoral fins and head and is regulated by retinoic acid. Mech Dev 65: 163–173.
- 33. Ogden JA (1976) Multiple hereditary osteochondromata. Report of an early case. Clin Orthop Relat Res 48–60.
- 34. Mansoor A, Beals RK (2007) Multiple exostosis: a short study of abnormalities near the growth plate. J Pediatr Orthop B 16: 363–365.
- 35. Hilton MJ, Gutierrez L, Martinez DA, Wells DE (2005) EXT1 regulates chondrocyte proliferation and differentiation during endochondral bone development. Bone 36: 379–386.
- 36. Koziel L, Kunath M, Kelly OG, Vortkamp A (2004) Ext1-dependent heparan sulfate regulates the range of Ihh signaling during endochondral ossification. Dev Cell 6: 801–813.
- 37. Stickens D, Zak BM, Rougier N, Esko JD, Werb Z (2005) Mice deficient in Ext2 lack heparan sulfate and develop exostoses. Development 132: 5055–5068.
- 38. Lin X, Wei G, Shi Z, Dryer L, Esko JD, et al. (2000) Disruption of gastrulation and heparan sulfate biosynthesis in EXT1-deficient mice. Dev Biol 224: 299–311.
- 39. Rauch GJ, Hammerschmidt M, Blader P, Schauerte HE, Strahle U, et al. (1997) Wnt5 is required for tail formation in the zebrafish embryo. Cold Spring Harb Symp Quant Biol 62: 227–234.
- 40. Cool SM, Nurcombe V (2005) The osteoblast-heparan sulfate axis: control of the bone cell lineage. Int J Biochem Cell Biol 37: 1739–1745.
- 41. Lemos MC, Kotanko P, Christie PT, Harding B, Javor T, et al. (2005) A novel EXT1 splice site mutation in a kindred with hereditary multiple exostosis and osteoporosis. J Clin Endocrinol Metab 90: 5386–5392.
- 42. Di Ferrante N, Ginsberg LC, Donnelly PV, Di Ferrante DT, Caskey CT (1978) Deficiencies of glucosamine-6-sulfate or galactosamine-6-sulfate sulfatases are responsible for different mucopolysaccharidoses. Science 199: 79–81.
- 43. Franco B, Meroni G, Parenti G, Levilliers J, Bernard L, et al. (1995) A cluster of sulfatase genes on Xp22.3: mutations in chondrodysplasia punctata (CDPX) and implications for warfarin embryopathy. Cell 81: 15–25.
- 44. ul Haque MF, King LM, Krakow D, Cantor RM, Rusiniak ME, et al. (1998) Mutations in orthologous genes in human spondyloepimetaphyseal dysplasia and the brachymorphic mouse. Nat Genet 20: 157–162.
- 45. Goda E, Kamiyama S, Uno T, Yoshida H, Ueyama M, et al. (2006) Identification and characterization of a novel Drosophila 3′-phosphoadenosine 5′-phosphosulfate transporter. J Biol Chem 281: 28508–28517.
- 46. Nüsslein-Volhard C, Dahm R (2002) Zebrafish : a practical approach. Oxford: Oxford University Press..
- 47. Knapik EW (1998) MGH/CVRC Zebrafish Server. Massachusetts General Hospital
- 48. Geisler R, Haffter P (1998) Tübingen Map of the Zebrafish Genome. Max-Planck-Institut für Entwicklungsbiologie
- 49. Sachdev SW, Dietz UH, Oshima Y, Lang MR, Knapik EW, et al. (2001) Sequence analysis of zebrafish chondromodulin-1 and expression profile in the notochord and chondrogenic regions during cartilage morphogenesis. Mech Dev 105: 157–162.
- 50. Yan YL, Hatta K, Riggleman B, Postlethwait JH (1995) Expression of a type II collagen gene in the zebrafish embryonic axis. Dev Dyn 203: 363–376.
- 51. Avaron F, Hoffman L, Guay D, Akimenko MA (2006) Characterization of two new zebrafish members of the hedgehog family: atypical expression of a zebrafish indian hedgehog gene in skeletal elements of both endochondral and dermal origins. Dev Dyn 235: 478–489.
- 52. Rentzsch F, Zhang J, Kramer C, Sebald W, Hammerschmidt M (2006) Crossveinless 2 is an essential positive feedback regulator of Bmp signaling during zebrafish gastrulation. Development 133: 801–811.
- 53. Yan YL, Miller CT, Nissen RM, Singer A, Liu D, et al. (2002) A zebrafish sox9 gene required for cartilage morphogenesis. Development 129: 5065–5079.