* Your assessment is very important for improving the workof artificial intelligence, which forms the content of this project
Download Fulltext - Jultika
Metagenomics wikipedia , lookup
Cell-free fetal DNA wikipedia , lookup
Population genetics wikipedia , lookup
No-SCAR (Scarless Cas9 Assisted Recombineering) Genome Editing wikipedia , lookup
Genetic engineering wikipedia , lookup
Gene desert wikipedia , lookup
Vectors in gene therapy wikipedia , lookup
History of genetic engineering wikipedia , lookup
Epigenetics of diabetes Type 2 wikipedia , lookup
Public health genomics wikipedia , lookup
Gene therapy of the human retina wikipedia , lookup
Nutriepigenomics wikipedia , lookup
Gene expression profiling wikipedia , lookup
Gene nomenclature wikipedia , lookup
Gene therapy wikipedia , lookup
Gene expression programming wikipedia , lookup
Genome evolution wikipedia , lookup
Saethre–Chotzen syndrome wikipedia , lookup
Genome editing wikipedia , lookup
Microsatellite wikipedia , lookup
Oncogenomics wikipedia , lookup
Therapeutic gene modulation wikipedia , lookup
Epigenetics of neurodegenerative diseases wikipedia , lookup
Genome (book) wikipedia , lookup
Neuronal ceroid lipofuscinosis wikipedia , lookup
Helitron (biology) wikipedia , lookup
Site-specific recombinase technology wikipedia , lookup
Frameshift mutation wikipedia , lookup
Designer baby wikipedia , lookup
Artificial gene synthesis wikipedia , lookup
FROM RARE SYNDROMES TO A COMMON DISEASE Mutations in minor cartilage collagen genes cause Marshall and Stickler syndromes and intervertebral disc disease SUSANNA ANNUNE N Department of Medical Biochemistry OULU 1999 SUSANNA ANNUNEN FROM RARE SYNDROMES TO A COMMON DISEASE Mutations in minor cartilage collagen genes cause Marshall and Stickler syndromes and intervertebral disc disease Academic Dissertation to be presented with the assent of the Faculty of Medicine, University of Oulu, for public discussion in the Auditorium of the Department of Medical Biochemistry, on December 3rd, 1999, at 12 noon. O U L U N Y L I O P I S TO , O U L U 1 9 9 9 Copyright © 1999 Oulu University Library, 1999 Manuscript received 01 October 1999 Accepted 13 October 1999 Communicated by Docent Jaakko Ignatius Professor Markku Savolainen ISBN 951-42-5413-9 (URL: http://herkules.oulu.fi/isbn9514254139/) ALSO AVAILABLE IN PRINTED FORMAT ISBN 951-425412-0 ISSN 0355-3221 (URL: http://herkules.oulu.fi/issn03553221/) OULU UNIVERSITY LIBRARY OULU 1999 Annunen, Susanna, From rare syndromes to a common disease. Mutations in minor cartilage collagen genes cause Marshall and Stickler syndromes and intervertebral disc disease. Collagen Research Unit, Biocenter Oulu and Department of Medical Biochemistry, University of Oulu, FIN-90220 Oulu, Finland 1999 Oulu, Finland (Received 1 October 1999) Abstract Collagens IX and XI are quantitatively minor components of the collagen fibrils in cartilage. The spectrum of the phenotypes caused by mutations in the COL2A1 gene coding for collagen II, the main cartilage collagen, is relatively well defined, but there is little data on the phenotypes caused by collagen IX and XI mutations. The structure of the human COL11A1 gene coding for the α1 chain of collagen XI was characterized here. It was found to consist of 68 exons and span 160 kb, excluding introns 1 and 4. Over 50 kb of new intronic sequences were defined. The exon-intron organization coding for the major triple helical domain was found to be identical to that of the human COL11A2 gene, which codes for the α2 chain of collagen XI. The sensitivity of conformation sensitive gel electrophoresis (CSGE) for mutation detection was improved and tested with a large number of sequence variations in collagen genes. The sensitivity with the revised conditions was found to be close to 100%. In addition, CSGE was found to be a simple and practical method for analyzing large numbers of samples. Fifteen mutations in the COL11A1 gene and eight in the COL2A1 gene were found by CSGE in patients with Marshall or Stickler syndrome. The genotypic-phenotypic comparison indicated that mutations leading to a premature translation termination codon in the COL2A1 gene resulted in Stickler syndrome and splicing mutations of 54 bp exons in the C terminal half of the COL11A1 gene resulted in Marshall syndrome. The other COL11A1 mutations caused phenotypes overlapping both syndromes. In an analysis of the COL9A2 gene in 157 patients with intervertebral disc disease, six were found to have a tryptophan for glutamine substitution in the central collagenous domain of the collagen IX molecule. None of 174 control individuals had this substitution. The substitution cosegregated with the phenotype in the families studied, and linkage and linkage disequilibrium analyses supported the association of the locus and the disease with a joint lod score of over 11. Keywords: mutation detection, sciatica Acknowledgements The research presented in this thesis was performed at the Department of Medical Biochemistry, University of Oulu, and Biocenter Oulu, Finland, and at the Center for Gene Therapy, the late Allegheny University of the Health Sciences, Philadelphia, USA, during the last years of the second millenium Anno Domini. I wish to express my sincere thanks to my supervisor, Docent Leena Ala-Kokko, for always having time to advise me, and sometimes even to help in the practical lab work, for her everlasting optimism, for arranging an opportunity for me to work at the Center for Gene Therapy in Philadelphia for two summers, and most importantly, for guiding me into the field of science. I would also like to thank Professors Kari I. Kivirikko and Taina Pihlajaniemi, the leaders of the Collagen Research Unit, for providing excellent research facilities and a high-standard scientific environment. Moreover, I wish to acknowledge Professor Ilmo Hassinen, whose enormous knowledge and enthusiastic attitude towards science inspired me as a first-year medical student to want to learn and create a piece of the fascinating world of science. I also wish to express my gratitude to Professor Darwin J. Prockop, Director of the Center for Gene Therapy, for giving me the honour of working in his laboratory. I am grateful to Professor Markku Savolainen and Docent Jaakko Ignatius for their valuable comments on the manuscript of this thesis. I also wish to thank Malcolm Hicks, M.A., for reviewing the language of the manuscripts of this thesis and the original articles II and III. I am indebted to all my collaborators. The clinicians who examined the patients and took samples made an invaluable contribution to this research. I also learned a lot about medicine from them. Harald H. H. Göring did much invaluable work in calculating the lod scores and trying to make me understand even something of the statistical dimensions. My friends and colleagues at the Department of Medical Biochemistry deserve my warmest thanks. The fruitful and relaxing scientific and non-scientific conversations and the time spent outside the lab with Jarmo Körkkö, Petteri Paassilta, Tero Pihlajamaa, Jussi and Mirka Vuoristo, Miia Melkoniemi, Merja Välkkilä, Merja Perälä, Jaana Lohiniva, Veli-Antero Kaakinen and Joni Mäki have been of great value for me. I also wish to thank Tero for teaching me the basics of lab work in the very first steps of this research and Miia for helping me to keep pace with my medical studies. Special thanks are due to Jarmo and Jaana Körkkö for their invaluable help in numerous things and all the moments of leisure spent with them during my stays in Philadelphia. My sister and colleague Pia Marttila deserves the greatest thanks for much wise advice concerning practical work and the more tortuous sides of scientific life. I wish to thank Aira Harju, Helena Lindqvist, Jaana Körkkö and Robert Hnatuk for their skilful technical assistance, Pertti Vuokila for ordering all the reagents and Seppo Lähdesmäki for helping with technical problems. I am grateful to Marja-Leena Kivelä and Auli Kinnunen for their always friendly secretarial help. I also wish to acknowledge Ari-Pekka Kvist and Juha Näpänkangas for maintaining the computer systems at the department and helping with the problems concerning computers. I wish to express my gratitude to my parents for their loving care and support and for giving me an excellent basis for my life. I am also grateful to my sisters, brother, their families and my friends for always being there for me even if I seemed to be constantly in the lab. Above all, I owe my deepest gratitude to my fiancé Markku for all his love, support and understanding and for brightening the dark moments and making the bright moments even brighter. This work was supported financially by the Emil Aaltonen Foundation and the Finnish Medical Foundation. Oulu, September 1999 Abbreviations 4Hyp ACGII-HCG BAP bp C cDNA COL COLyAx Colyax COMP CSGE CT DGGE ECM FACIT GAG kb kDa MACIT MED MRI mRNA MULTIPLEXIN N NC OA OMIM OSMED PSACH RT-PCR SED SSCP 4-hydroxyproline achondrogenesis type II-hypochondrogenesis 1,4-bis(acryloyl)piperazine basepair carboxy complementary DNA collagenous domain human gene for the α(x) chain of collagen y murine gene for the α(x) chain of collagen y cartilage oligomeric matrix protein conformation sensitive gel electrophoresis computerized tomography denaturing gradient gel electrophoresis extracellular matrix fibril-associated collagen with interrupted triple helices glycosaminoglycan kilobase kilodalton membrane-associated collagen with interrupted triple helices multiple epiphyseal dysplasia magnetic resonance imaging messenger RNA collagen with multiple triple helix domains and interruptions amino non-collagenous domain osteoarthritis or osteoarthrosis Online Mendelian Inheritance in Man otospondylomegaepipyseal dysplasia pseudoachondroplasia reverse transcriptase PCR spondyloepiphyseal dysplasia single-strand conformation polymorphism WZS X Y Weissenbacher-Zweymüller syndrome any amino acid any amino acid List of original articles This thesis is based on the following articles, which are referred to in the text by their Roman numerals: I Körkkö J, Annunen S, Pihlajamaa T, Prockop DJ & Ala-Kokko L (1998) Conformation sensitive gel electrophoresis for simple and accurate detection of mutations: comparison with denaturing gradient gel electrophoresis and nucleotide sequencing. Proc Natl Acad Sci USA 95: 1681-1685. II Annunen S, Körkkö J, Czarny M, Warman ML, Brunner HG, Kääriäinen H, Mulliken JB, Tranebjærg L, Brooks DG, Cox GF, Cruysberg JR, Curtis MA, Davenport SLH, Friedrich CA, Kaitila I, Krawczynski MR, Latos-Bielenska A, Mukai S, Olsen BR, Shinno N, Somer M, Vikkula M, Zlotogora J, Prockop DJ & Ala-Kokko L (1999) Splicing mutations of 54 bp exons in the COL11A1 gene cause Marshall syndrome but other mutations cause overlapping Marshall/Stickler phenotypes. Am J Hum Genet 65: 974-983. III Annunen S, Paassilta P, Lohiniva J, Perälä M, Pihlajamaa T, Karppinen J, Tervonen O, Kröger H, Lähde S, Vanharanta H, Ryhänen L, Göring HHH, Ott J, Prockop DJ & Ala-Kokko L (1999) An allele of COL9A2 associated with intervertebral disease. Science 285: 409-412. In addition, some unpublished data are presented. Contents Abstract Acknowledgements Abbreviations List of original articles Contents 1. Introduction.................................................................................................................. 13 2. Review of the literature................................................................................................ 15 2.1. Collagens............................................................................................................... 15 2.1.1. Fibrillar collagens........................................................................................ 15 2.1.2. Non-fibrillar collagens ................................................................................ 16 2.1.3. Collagen biosynthesis.................................................................................. 18 2.2. Cartilage................................................................................................................ 18 2.2.1. Collagenous components of cartilage.......................................................... 19 2.2.2. Non-collagenous components of cartilage .................................................. 22 2.3. Cartilage collagens in non-cartilaginous tissues ................................................... 23 2.3.1. Inner ear ...................................................................................................... 23 2.3.2. Ocular vitreous body ................................................................................... 23 2.3.3. Intervertebral disc........................................................................................ 23 2.4. Disorders affecting cartilage collagens ................................................................. 24 2.4.1. Achondrogenesis type II-hypochondrogenesis (ACGII-HCG) ................... 25 2.4.2. Spondyloepiphyseal dysplasia (SED).......................................................... 25 2.4.3. Kniest dysplasia........................................................................................... 26 2.4.4. Stickler and Marshall syndromes ................................................................ 26 2.4.5. Otospondylomegaepiphyseal dysplasia (OSMED), WeissenbacherZweymüller syndrome (WZS) and non-ocular Stickler-like syndrome....... 28 2.4.6. Multiple epiphyseal dysplasia (MED)......................................................... 29 2.4.7. Osteoarthritis (OA)...................................................................................... 30 2.5. Animal models for disorders of the cartilage collagens ........................................ 30 2.5.1. Collagen II................................................................................................... 31 2.5.2. Collagen IX ................................................................................................. 31 2.5.3. Collagen XI ................................................................................................. 32 2.6. Intervertebral disc disease..................................................................................... 32 2.6.1. Cmd mice .................................................................................................... 33 2.7. Mutation detection methods.................................................................................. 33 2.7.1. Commonly used methods based on electrophoresis .................................... 33 2.7.2. Commonly used methods based on cleavage of a mismatch....................... 34 2.7.3. Other methods ............................................................................................. 35 3. Outlines of the present research ................................................................................... 37 4. Materials and methods ................................................................................................. 38 4.1. Subjects and clinical examination methods (I-III) ................................................ 38 4.2. Characterization of the COL11A1 gene (II).......................................................... 39 4.3. CSGE (I-III) .......................................................................................................... 39 4.4. Screening of the COL11A1 and COL2A1 genes of patients with Marshall and Stickler syndromes for mutations by CSGE (II) ................................................... 40 4.5. RT-PCR (II) .......................................................................................................... 41 4.6. Screening of patients with sciatica for mutations in the COL9A2 gene (III) ........ 41 4.7. Statistical analysis (III) ......................................................................................... 41 5. Results.......................................................................................................................... 43 5.1. Optimization of CSGE (I) ..................................................................................... 43 5.1.1. Improved conditions for mutation detection by CSGE (I) .......................... 43 5.1.2. Testing the sensitivity and specificity of CSGE.......................................... 44 5.2. Characterization of the human COL11A1 gene (II).............................................. 44 5.2.1. Characterization of clones for the COL11A1 gene ..................................... 45 5.2.2. Genomic structure of the human COL11A1 gene ....................................... 45 5.2.3. Resequencing of the coding region ............................................................. 46 5.3. Identification of mutations in the COL11A1 and COL2A1 genes in patients with Marshall or Stickler syndrome (II)................................................................ 46 5.3.1. Identification of mutations in the COL11A1 and COL2A1 genes by CSGE........................................................................................................... 46 5.3.2. Genotypic-phenotypic comparison.............................................................. 47 5.4. Identification of an allele of the COL9A2 gene associated with intervertebral disc disease (III) .................................................................................................... 50 5.4.1. Identification of a tryptophan for glutamine/arginine substitution in the COL9A2 gene.............................................................................................. 50 5.4.2. Co-inheritance of the Trp allele and intervertebral disc disease.................. 50 5.4.3. Statistical analysis ....................................................................................... 50 5.4.4. Scanning the entire COL9A2 gene for mutations in patients with the Trp allele ............................................................................................................ 52 6. Discussion.................................................................................................................... 53 6.1. Detection of mutations by CSGE .......................................................................... 53 6.2. Genomic structure of the human COL11A1 gene................................................. 54 6.3. COL11A1 and COL2A1 gene mutations in patients with Marshall or Stickler syndrome ............................................................................................................... 55 6.4. The association of a COL9A2 allele with intervertebral disc disease ................... 57 7. References.................................................................................................................... 59 1. Introduction Cartilage is an important form of supportive tissue. It is rich in extracellular matrix and contains only a sparse population of chondrocytes. The most abundant type of cartilage in the body is hyaline cartilage, which forms articular cartilage, growth plates and the cartilaginous anlage for endochondral ossification. The extracellular matrix of hyaline cartilage is highly hydrated and comprises cartilage-specific collagen fibrils and proteoglycans. Collagen II, the main component of the collagen fibrils in cartilage, is a homotrimer of three identical α chains, α1(II)3, which are encoded by the COL2A1 gene. While collagen II accounts for the majority of the collagens in cartilage, other significant types are collagens IX and XI. Collagen IX is a heterotrimer of three dissimilar α chains, α1(IX), α2(IX) and α3(IX), which are encoded by the COL9A1, COL9A2 and COL9A3 genes, respectively. Collagen IX is known to be located on the surface of the cartilage collagen fibrils, but its precise function is not currently known, although it has been suggested that it may mediate the interaction between collagenous and non-collagenous cartilage components and maintain the homeostasis of cartilage. Collagen XI is likewise a heterotrimer of three distinct α chains, the α1(XI), α2(XI) and α3(XI) chains being encoded by the COL11A1, COL11A2 and COL2A1 genes, respectively. Like collagen II, collagen XI forms fibrils, and they are thought to be buried in collagen II fibrils. It has been suggested that the function of collagen XI may be to regulate collagen fibril diameter. Collagens II, IX and XI are also expressed in the intervertebral disc, which consists of an outer ring-like structure called the annulus fibrosus and an inner gel-like matrix called the nucleus pulposus. Collagen II is the major collagenous component of the nucleus pulposus, while collagen IX is found in minor amounts throughout the disc and collagen XI accounts for a few percent of the collagens in the nucleus pulposus. In addition to hyaline cartilage and the intervertebral disc, collagens II, IX and XI are also expressed in the ocular vitreous body and the tectorial membrane of the inner ear. Collagen II is the most intensively studied collagen type in cartilage, and a large number of mutations in the COL2A1 gene have already been characterized. Depending on the type of mutation, they cause a spectrum of phenotypes ranging from lethal achondrogenesis type II-hypochondrogenesis to early onset osteoarthritis with mild chondrodysplasia. Mutations characterized in the genes coding for collagen IX lead to 14 multiple epiphyseal dysplasia, and mutations in the genes coding for collagen XI lead to Stickler and Marshall syndromes and heterozygous and homozygous otospondylomegaepiphyseal dysplasia. The number of mutations in these genes known at present is small, however, and the spectrum of phenotypes caused by gene mutations in collagens IX and XI is largely unknown. Characterization of the genetic defects lying behind such phenotypes is important for obtaining an understanding of the function of the particular molecule and of the whole tissue. Furthermore, knowing the molecular defect that causes the disorder in question helps in the development of a treatment for the disease and the prevention of symptoms, and on the other hand, enables defining the exact genetic defect involved and genetic prenatal diagnosis. The goal of this thesis is to increase our knowledge of the role of collagens IX and XI in disorders affecting cartilaginous tissues. It involves characterization of the genomic structure of the COL11A1 gene, the description of 23 mutations in the COL11A1 and COL2A1 genes causing Marshall and Stickler syndromes, definitions of the genotypic and phenotypic relations of these syndromes, and a report of an association between an allele of the COL9A2 gene bearing a putative mutation and intervertebral disc disease. In addition, an improvement to the conformation sensitive gel electrophoresis (CSGE) method for mutation detection is described. 2. Review of the literature 2.1. Collagens Collagens are a significant component of the extracellular matrix (ECM). They are a group of related proteins that share common structural characteristics. Collagens are trimeric molecules consisting of three similar or dissimilar α chains, and they form supramolecular structures in the ECM. All collagens have at least one triple helical region in the molecule. The formation of triple helix requires the presence of glycine as every third amino acid, because any bulkier amino acid would cause steric hindrance to helix formation. So far, 19 collagen types encoded by over 30 different genes are known. These can be divided into several groups based on their structural and other properties (For reviews, see Vuorio & de Crombrugghe 1990, Kielty et al. 1993, Mayne & Brewton 1993, Pihlajaniemi & Rehn 1995, Prockop & Kivirikko 1995.) 2.1.1. Fibrillar collagens Collagens I, II, III, V and XI aggregate into rod-like fibrils in a quarter-staggered array that gives a characteristic banding pattern. They contain a large collagenous domain of about 1000 amino acids. (See Kielty et al. 1993, Pihlajaniemi & Rehn 1995, Prockop & Kivirikko 1995.) Collagens I, II and III are known as the major fibrillar collagens, since they are quantitatively more significant than collagens V and XI, which are often called minor fibrillar collagens. Collagen I, II and III fibrils create the structural frameworks for many tissues, such as bone, skin, cartilage, tendon and blood vessels. Collagen I is a heterotrimer of two α1(I) chains and one α2(I) chain that are encoded by the COL1A1 and COL1A2 genes, respectively. Homotrimers of α1(I) have also been observed (Uitto 1979). Collagen I is expressed in various tissues, but it is the main structural component of bone, skin, tendon, ligament, teeth and fasciae. Collagen II is a homotrimer of α1(II) chains that are encoded by the COL2A1 gene. In adult tissues it is expressed in cartilage, vitreous humour, the intervertebral disc and the inner ear (for more details on collagen II, see section 2.2.1.1.). 16 Collagen III is a homotrimer as well, consisting of three α1(III) chains that are encoded by the COL3A1 gene and being expressed in various tissues, although it is most abundant in elastic tissues such as the skin, blood vessels, gut and lung. The major fibrillar collagens share highly similar characteristics. They are synthesized as large precursors with C and N propeptides, which are later cleaved by specific C and N proteinases. Also, all the genes coding for the α chains of major fibrillar collagens are similar in their genomic structure. The numbers and the sizes of the exons are the same, with only a few exceptions. (See Vuorio & Crombrugghe 1990, Chu & Prockop 1993, Prockop & Kivirikko 1995.) Collagens V and XI share many properties with the major fibrillar collagens, although they also have some features that are different. The exon sizes and numbers of exons in the genes for the minor fibrillar collagens characterized so far, the COL5A1 and COL11A2 genes, are different from those of the genes that code for the major fibrillar collagens (Takahara et al. 1995, Vuoristo et al. 1995). While the entire propeptides are cleaved during post-translational modification in the major fibrillar collagens, the N propeptides of collagens V and XI seem to be partially retained in the mature molecule. Collagens V and XI form heterotypic fibrils with collagens I and II, respectively, and they are thought to be located inside collagen I/II fibrils (Birk et al. 1988, Mendler et al. 1989). It has been suggested that they regulate fibril diameter and thus have a significant role in fibril formation. Collagen V is codistributed with collagen I, and is composed of three different α chains, α1(V), α2(V) and α3(V), encoded by the COL5A1, COL5A2 and COL5A3 genes. The most common composition for the collagen V molecule is [α1(V)]2α2(V), but others also exist. Collagen XI usually consists of α1(XI), α2(XI) and α3(XI) chains, coded by the COL11A1, COL11A2 and COL2A1 genes (for more details on collagen XI, see section 2.2.1.3.). Collagen V and XI α chains can also appear in the same heterotypic molecule, e.g. the α2(V) chain substitutes for α2(XI) in the vitreous body of the eye. It has therefore been suggested that collagens V and XI could be considered a single type, collagen V/XI. (See Fichard et al. 1994.) 2.1.2. Non-fibrillar collagens Of the currently known collagen types, collagens IV, VI-X and XII-XIX are the ones that do not form fibrils. According to their structural properties, they can be further classified as network-forming collagens, beaded filament-forming collagen, collagen of anchoring fibrils, fibril-associated collagens with interrupted triple helices (FACITs), membraneassociated collagens with interrupted triple helices (MACITs) and collagens with multiple triple helix domains and interruptions (MULTIPLEXINs) (see Pihlajaniemi & Rehn 1995, Prockop & Kivirikko 1995). Collagens IV, VIII and X form network-like structures. Collagen IV has a large triple helical domain that is interrupted by numerous short non-collagenous sequences, which confer flexibility on the individual molecule. This allows aggregation of the monomers to form the network-like structures that are found in basement membranes. The structures of collagens VIII and X are very similar to each other but differ from that of collagen IV. The triple helical domains of collagens VIII and X are only about 450 amino acids in 17 length and these types assemble into hexagonal lattices. The genes that code for collagens VIII and X have an atypical structure, since they consist of only three exons, the third of which codes for almost the entire protein. Collagen VIII is expressed primarily in Descemet’s membrane in the eye, and collagen X is a highly specialized collagen of hypertrophic chondrocytes in the deep-calcifying zone of cartilage. (See Kielty et al. 1993, Pihlajaniemi & Rehn 1995, Prockop & Kivirikko 1995.) Collagen VI molecules form a unique structure of beaded filaments, which are found in most connective tissues. It is located in the close vicinity of cells, large collagen fibrils and some basement membranes, and may thus function as an anchorage between these structures and the surrounding ECM. (See Chu et al. 1990.) Collagen VII is the major component of the anchoring fibrils that attach the basement membrane to the stroma of the tissues, subject to external frictional forces such as skin, oral mucosa and cervix (see Burgeson et al. 1990, Kielty et al. 1993). The FACITs (IX, XII, XIV, XVI, XIX) do not form fibrils themselves, but are found to be associated with fibrillar collagens. They are not secreted as procollagens like the fibrillar collagens are, and thus do not undergo proteolytic processing after secretion. (See Shaw & Olsen 1991, Mayne & Brewton 1993, Prockop & Kivirikko 1995.) Collagen IX, the best studied member of the FACIT group, is expressed in the same tissues as collagen II and is covalently crosslinked to the surface of collagen II fibrils (Eyre et al. 1987, Brewton & Mayne 1994, Diab et al. 1996; for more details on collagen IX, see chapter 2.2.1.2.). Collagens XII and XIV bear structural similarities to collagen IX, but their functions are unclear, although it has been suggested that they are associated with collagen I fibrils. There is also evidence of collagen XII and XIV expression in tissues from which collagen I is absent, however. Collagens XVI and XIX have also been classified as FACITs in view of their homology with the other FACITs. (See Mayne & Brewton 1993.) Even though the exact function of the FACITs is unclear, it has been suggested that they may serve as molecular bridges and thus have a role in ECM organization and integrity (see Shaw & Olsen 1991). Collagens XIII and XVII are not homologous in structure but have a transmembrane domain, and are therefore called MACITs. The mRNA for collagen XIII can be found in a variety of tissues, but the function of the protein has not yet been defined. Even though alternative splicing is relatively common in collagens, that found in collagen XIII is of an unusual complexity, affecting the sequences for ten exons. Collagen XVII is expressed in hemidesmosomes of the skin. Autoantibodies against it have been identified in cases of bullous pemphigoid, an autoimmune disease that causes blistering, suggesting an anchoring function for this collagen. (See Pihlajaniemi & Rehn 1995.) Collagens XV and XVIII consist of multiple triple helical domains and interruptions and are thus called MULTIPLEXINs. They are homologous proteins that are expressed in a variety of tissues, with overlapping but not similar distributions (Kivirikko et al. 1995, Saarela et al. 1998). A fragment of the C terminus of collagen XVIII is proteolytically cleaved to form endostatin, which is known to prevent angiogenesis (O’Reilly et al. 1997). 18 2.1.3. Collagen biosynthesis After the transcription and translation of collagen mRNA, the newly synthesized polypeptide undergoes post-translational modifications both intracellularly, in the endoplasmic reticulum, and extracellularly. The biosynthesis of collagen is a complex multistage process that requires numerous enzymes. Following cleavage of the signal peptide, prolyl residues in X-Pro-Gly sequences are hydroxylated to hydroxyprolines, lysyl residues in X-Lys-Gly sequences to hydroxylysines, and prolyl residues in Pro4Hyp-Gly sequences to hydroxyprolines by the enzymes prolyl 4-hydroxylase, lysyl hydroxylase and prolyl 3-hydroxylase, respectively. Prolyl 4-hydroxylase plays a central role in collagen biosynthesis, since 4-hydroxyproline is essential for triple helix stability at body temperature. Some of the hydroxylysyl residues are further glycosylated with galactose or galactose and glucose by hydroxylysyl galactosyl transferase or galactosyl hydroxylysyl glucosyl transferase, respectively. The formation of the triple helix proceeds from the C terminus to the N terminus. The initial interaction between the noncollagenous domains of the α chains leads to nucleation of the C termini of the collagenous domains and then to the propagation of triple helix formation in a zipper-like manner. Correct chain selection is directed by molecular recognition sequences in the C terminal non-collagenous domains (Lees et al. 1997). In addition, interchain disulphide bonds in the C terminal non-collagenous domains, catalyzed by protein disulphide isomerase (PDI), stabilize the chain assembly, but they are not essential for triple helix formation (Bulleid et al. 1996, see also Bulleid 1996). The correctly folded procollagen molecules are secreted through the Golgi complex. (See Kielty et al. 1993, Kivirikko 1995, Prockop & Kivirikko 1995.) The C and N propeptides are cleaved from the procollagen molecules by specific C and N proteinases in the extracellular space, removal of the propeptides being a requirement for normal fibril formation. The cleavage of the propeptides converts the soluble procollagen molecules to insoluble collagen molecules that are able to selfassemble and form fibrils spontaneously. The fibril-forming collagens undergo this cleavage through the action of C and N proteinases, but many of the non-fibrillar collagens retain the C and N terminal non-collagenous domains in the mature molecule. After aggregation of the collagen molecules into fibrils, covalent cross-links are formed to provide the supramolecular structures with tensile strength and mechanical stability. The cross-links are formed either by disulphide bonds between cysteine residues or by lysyl and hydroxylysyl aldehydes that are formed in the reaction catalyzed by lysyl oxidase. (See Kielty et al. 1993, Kivirikko 1995.) 2.2. Cartilage Cartilage is hyperhydrated supportive tissue that does not contain blood vessels, nerves or lymphatics. It consists of about 80% water by weight, and the remaining 20% is mainly collagen II and proteoglycans. Cartilage is rich in ECM, which is produced by chondrocytes of mesenchymal origin. There are three types of cartilage. Hyaline cartilage is the prototypic manifestation that forms articular cartilage, the cartilaginous anlage of 19 developing bones, the epiphyseal plates, the costochondral cartilages and the cartilages of the respiratory tract. Fibrocartilage resembles hyaline cartilage but contains collagen I fibres for tensile and structural strength. It is found in the annulus fibrosus of the intervertebral disc, tendinous and ligamentous insertions, menisci, the symphysis pubis and the insertions of joint capsules. Elastic cartilage constitutes the pinna of the ears, the epiglottis and the arytenoid cartilages of the larynx. (See Schiller 1994, Muir 1995.) 2.2.1. Collagenous components of cartilage Collagens provide the structural framework for hyaline cartilage. Collagen II, which constitutes 80-85% of the total collagen content of cartilage, forms fibrils that contain small amounts of collagens IX and XI. The quantities of these minor cartilage collagens range from 1% to 10%, depending on the cartilage source and age. Small amounts of collagens VI, XII and XIV have also been identified in cartilage. Expression of collagen X is restricted to hypertrophic chondrocytes during endochondral ossification. (See Mayne 1989, Eyre 1991, Brewton & Mayne 1994, Eyre & Wu 1995, Cremer et al. 1998.) 2.2.1.1. Collagen II The COL2A1 gene that codes for the α chains of homotrimeric collagen II consists of 54 exons and is about 31 kb in size (Ala-Kokko & Prockop 1990, Ala-Kokko et al. 1995). Its chromosomal location is 12q13.11-q13.12 (Takahashi et al. 1990). Besides its expression in cartilage, the ocular vitreous body, intervertebral discs and the inner ear, collagen II can be found in many non-chondrogenic tissues during development (see Brewton & Mayne 1994). The sequences coding for the N terminal propeptide contain an alternatively spliced exon that codes for a 69-amino acid cysteine-rich domain (Ryan & Sandell 1990). Collagen II molecules including (IIA) or excluding this domain (IIB) have distinct distributions in the stages of chondrogenesis, type IIA predominating in the prechondrogenic mesenchyme and differentiating chondrocytes, and type IIB in differentiated chondrocytes (Nah & Upholt 1991, Sandell et al. 1991). The collagen II molecules in the fibril overlap with each other by a distance of about a quarter of their length, thus forming a banded fibril. The molecules are covalently crosslinked between the triple helical domain and the N or C terminal telopeptides of adjacent collagen II molecules, i.e. the short non-collagenous regions that are retained in propeptide cleavage. The particular molecular properties that serve to adapt the collagen for use in cartilage are unclear, but it has been suggested that the high hydroxylysine content of the molecule results in a highly hydrated fibril suitable for cartilage. (See Eyre 1991, Kielty et al. 1993, Eyre & Wu 1995.) 20 2.2.1.2. Collagen IX Collagen IX is a heterotrimeric molecule composed of three separate gene products, α1(IX), α2(IX) and α3(IX) chains. Like collagen II, it is expressed in cartilage, the ocular vitreous body, intervertebral discs and the inner ear (Ayad et al. 1982, Slepecky et al. 1992b, see also Brewton & Mayne 1994). Collagen IX belongs to the group of FACITs and consists of three collagenous (COL1-COL3) and four non-collagenous (NC1-NC4) domains numbered from the C terminus of the molecule. The length of the molecule is about two-thirds of that of the collagen II molecule. (See Kielty et al. 1993.) The molecule is covalently crosslinked to the surface of collagen II fibrils in an antiparallel manner; the N terminal regions of the COL2 domains of all three chains being crosslinked to the N telopeptide of α1(II) and the central region of the COL2 domain of α3(IX) chain to the C telopeptide of α1(II) (Eyre et al. 1987, Vaughan et al. 1988, Wu et al. 1992, Diab et al. 1996). In addition, collagen IX molecules have been shown to be crosslinked to one another between the N terminal COL2 domain of the α1(IX) or α3(IX) chain and the C terminal NC1 domain of the α3(IX) chain (Wu et al. 1992, Diab et al. 1996). The length of the NC3 domain is different in all three α chains, thus forming a kink in the molecule (McCormick et al. 1987). When the COL2 domain is attached covalently to the surface of collagen II fibrils, the kink allows the COL3 and NC4 domains to project away from the fibril surface (Bruckner et al. 1988, Vaughan et al. 1988). Collagen IX can also be classified as proteoglycan, because the molecule contains a glycosaminoglycan (GAG) side chain (Bruckner et al. 1985, Bruckner et al. 1988). The attachment site for the chondroitin sulphate side chain is located in the NC3 domain of the α2(IX) chain (Huber et al. 1986, McCormick et al. 1987). The proportion of molecules with glycosaminoglycan side chain substitution varies depending on the tissue and its source, and the function of the glycosaminoglycan side chain is not known (Yada et al. 1990, Diab et al. 1996, see also Brewton & Mayne 1994). The α chains of collagen IX are encoded by the COL9A1, COL9A2 and COL9A3 genes. The COL9A2 and COL9A3 genes consist of 32 exons, while the COL9A1 gene consists of 38 exons. The six additional exons of the COL9A1 gene code for the 243amino-acid globular NC4 domain that is formed only from the α1(XI) chain. There is an alternative promoter and second transcription start site in the COL9A1 gene, giving rise to a short form of the α1(IX) chain and the whole collagen IX molecule. In the short form the alternative exon 1 in intron 6 is used and exon 7 is skipped, thus splicing the alternative exon 1 straight to exon 8 of the COL9A1 gene (Nishimura et al. 1989). The short form exists primarily in the eye. (See Brewton & Mayne 1994.) The exon-intron structures of the corresponding regions of these genes are highly similar, but the genes are very different in size. The COL9A1 gene spans about 90 kb, while the COL9A2 and COL9A3 genes are only about 15 and 23 kb, respectively. (Pihlajamaa et al. 1998a, Paassilta et al. 1999b.) The chromosomal locations of the genes are 6q12-q13 (COL9A1), 1p33-p32.2 (COL9A2) and 20q13.3 (COL9A3) (Warman et al. 1993b, Warman et al. 1994, Tiller et al. 1998). The function of collagen IX is not currently known. The location of collagen IX molecules on the surface of collagen II and the projection of the COL3 and NC4 domains out from the surface of the fibril suggest a role in the intermolecular organization of 21 cartilage. The pI of the NC4 domain is about 10, thus making the domain a candidate for interaction with the highly anionic glycosaminoglycans of cartilage (Vasios et al. 1988). There is also evidence of a role of collagen IX in the maintenance of cartilage integrity (Fässler et al. 1994, Hagg et al. 1998). 2.2.1.3. Collagen XI Collagen XI, originally called 1α2α3α collagen, is similarly a heterotrimer, and is quantitatively a minor member of the group of fibrillar collagens (Morris & Bächinger 1987). Like collagens II and IX, collagen XI is expressed in cartilage, the ocular vitreous body and the nucleus pulposus (see Eyre & Wu 1987, Brewton & Mayne 1994), but the question of its occurrence in the inner ear is controversial (Slepecky et al. 1992b, Thalmann 1993). Furthermore, the mRNAs for all the α(XI) chains can be found in equal or unequal amounts in a variety of tissues (Lui et al. 1995). The molecule consists of a major triple helical region of about 1000 amino acids (COL1) that is flanked by a noncollagenous C terminal region (NC1) and an N terminal region that consists of a minor triple helical region (COL2) flanked by non-collagenous domains (NC2 and NC3). Collagens V and XI seem to resemble each other closely in their structural and biological properties. In addition, their α chains can substitute for each other, so that a fraction of α1(XI) in cartilage has been replaced by α1(V) (see Eyre & Wu 1987) and a fraction α1(V) in bone has been replaced by α1(XI) (Niyibizi & Eyre 1989). Furthermore, the ocular vitreous body contains the α1(XI) and α2(V) chains but no α2(XI) chain (Mayne et al. 1993). These findings have led to the suggestion that collagens V and XI should be classified as a single collagen type, collagen V/XI. (See Fichard et al. 1994.) The α1(XI) and α2(XI) chains are products of the COL11A1 and COL11A2 genes, respectively, while the α3(XI) chain is an overglycosylated form of the IIB splicing variant product of the COL2A1 gene that also codes for the α chains of collagen II (Eyre & Wu 1987, Wu & Eyre 1995). The COL11A1 gene is located in the p21 region of chromosome 1 (Henry et al. 1988). The cDNA for it has been cloned, but only a minor fraction of the exon-intron organization has been elucidated (Bernard et al. 1988, Zhidkova et al. 1995). On the other hand, the genomic organization of the COL11A2 gene has been thoroughly defined. It spans 28 kb and consists of 66 exons. Even though it shares some properties of the major fibrillar collagens, there are marked differences in the number of exons, exon sizes and codon usage, indicating that the gene has not evolved with those for the major fibrillar collagens. (Vuoristo et al. 1995.) The COL11A2 gene is located at 6p21.2 (Kimura et al. 1989) or 6p21.3 (Hanson et al. 1989). Both the α1(XI) and α2(XI) chains undergo alternative splicing in the N terminal propeptide. The transcripts for the α1(XI) chain contain either exon IIA, coding for 39 amino acids, IIB coding for 51 amino acids, or neither of them, but not both. In addition, exon IV, coding for 85 amino acids, may or may not be present in the mRNA. It is notable that exons IIA, III and IV are highly acidic, while exon IIB is highly basic. The alternative splicing of the α2(XI) chain involves exons 6, coding for 26 amino acids, and 7, coding for 21 amino acids. Furthermore, Lui et al. (1996) suggest additional splicing of sequences in intron 6 of the transcript to the mRNA, yielding a truncated α2(XI) chain 22 because of the translation termination codons in the sequences. (Zhidkova et al. 1995.) The N terminal domain of the α2(XI) chain has also been shown to give rise to proline/arginine-rich protein (PARP) in cartilage (Neame et al. 1990, Zhidkova et al. 1993). Collagen XI molecules are covalently cross-linked primarily to each other in head to tail organization. The cross-links occur between the N telopeptides and the C terminal ends of the helical regions. In addition, the N terminal end of the α1(XI) chain is attached to the C telopeptide sequence of the α3(XI) or α1(II) chain, presumably to α1(II). These data indicate that collagen XI may form primarily homopolymers, which are also capable of cofibrillar assembly with collagen II. (Wu & Eyre 1995.) The coexistence of collagens II, IX and XI in the cartilage collagen fibrils and the finding that collagen XI is immunologically masked has led to the suggestion that collagen XI is buried inside the fibril (Mendler et al. 1989). Its hypothesized function is regulation of fibril diameter. This is supported by the finding that collagen XI is restricted to thin fibrils and that mouse and human defective collagen XI occurs in abnormal thick, disorganized fibrils (Seegmiller et al. 1971, Keene et al. 1995, Li Y et al. 1995, van Steensel et al. 1997). Partial retention of the N propeptide has been proposed as the molecular basis for this function. (See Fichard et al. 1994.) 2.2.2. Non-collagenous components of cartilage While collagens form the structural network for cartilage, proteoglycans (also called mucopolysaccharides) provide hydration and swelling pressure, enabling the cartilage to withstand compressional forces. Proteoglycans are proteins that have one or more GAG side chain, which may be chondroitin sulphate, dermatan sulphate, keratan sulphate, heparan sulphate or heparin. (See Hardingham & Fosang 1992, Roughley & Lee 1994.) The largest and most abundant proteoglycan in cartilage is aggrecan, which consists of a multidomain core protein of over 200 kDa bearing over a hundred chondroitin and keratan sulphate side chains in a bottle brush manner. The core protein of an aggrecan molecule attaches to hyaluronan by non-covalent binding, which is stabilized by link protein, thus forming huge multimolecular aggregates. (See Neame & Barry 1993, Hardingham & Fosang 1995.) Many other proteoglycans, such as decorin, biglycan, fibromodulin, lumican and PRELP (proline/arginine-rich end leucine-rich repeat protein), have also been characterized in cartilage. These have relatively small core proteins and only a few GAGs. While aggrecan is mainly responsible for the hydration of cartilage, other proteoglycans in cartilage have distinct biological functions apart from their hydrodynamic functions, e.g. regulation of collagen fibrillogenesis or cell adhesion and migration. (Grover et al. 1995, Bengtsson et al. 1995, Kinsella et al. 1997, see also Stanescu 1990, Roughley & Lee 1994.) In addition to link protein, there are other non-collagenous proteins in cartilage that do not belong to the proteoglycans, e.g. cartilage oligomeric matrix protein (COMP), anchorin and chondrocalcin in cartilage (see Heinegård & Oldberg 1989). 23 2.3. Cartilage collagens in non-cartilaginous tissues Besides cartilage, cartilage collagens are significant structural components of the tectorial membrane of the inner ear, the ocular vitreous body and intervertebral discs. 2.3.1. Inner ear Collagen II, which is the most studied cartilage collagen in the inner ear, has been found in various tissues there, such as the tectorial, basilar and vestibular membranes and the cartilaginous rest of the endochondral layer (Thalmann 1986, Slepecky et al. 1992b, Thalmann 1993). Thalmann et al. (1987) have shown that collagen accounts for approximately 40% of the total protein in the tectorial membrane of the guinea pig. This membrane lies over the organ of Corti, and the stereocilia of the outer hair cells are embedded in its gel-like matrix (see Moore 1992a). The co-localization of collagens II and IX in the thick, unbranched radial fibres of the tectorial membrane is well demonstrated, but there is some inconsistency in reports with regard to the expression of collagens XI and V in the tectorial membrane and in the inner ear generally (Slepecky et al. 1992a, Slepecky et al. 1992b, Thalmann 1993). 2.3.2. Ocular vitreous body The ocular vitreous body is a gel-like structure consisting primarily of hyaluronan and collagen fibrils (Ren et al. 1991, Brewton & Mayne 1992). The collagenous component comprises collagen II, collagen IX and collagen resembling types V and XI (Swann & Sotman 1980, Ayad et al. 1982, Ayad & Weiss 1984, Seery & Davison 1991). Further studies by Mayne et al. (1993) demonstrated that the chains of the collagen V/XI fraction of bovine vitreous body are α1(XI) and α2(V). Since neither of these is known to exist in homotrimers (see Fichard et al. 1994), it is highly probable that they form heterotypic trimers either with or without the α1(II) chain. Collagen IX in the vitreous lacks the NC4 domain, suggesting utilization of the alternative downstream promoter of the COL9A1 gene (Ren et al. 1991, Warman et al. 1993a). (See Brewton & Mayne 1994, Bishop 1996.) 2.3.3. Intervertebral disc An intervertebral disc stabilizes the spine by anchoring adjacent vertebral bodies to each other and simultaneously absorbs the compressive forces directed towards the spine. While stabilization of the spine requires firmness, resilience is essential for shock absorption. To fulfil both of these tasks, the intervertebral disc comprises concentrically arranged compartments. The outermost structure is a ring-like outer annulus fibrosus, 24 which consists of highly oriented, densely packed collagen fibril lamellae, inside which is the fibrocartilaginous inner annulus fibrosus. There is a transition zone separating the central nucleus pulposus, a gel-like structure, from the layers of the annulus fibrosus, and there are no clear boundaries between the structures of the intervertebral disc. The cartilaginous endplates between the vertebral bodies and the intervertebral disc are often considered part of the intervertebral disc. (See Humzah & Soames 1988, Moore 1992b, Buckwalter 1995.) Collagens I and II are the predominant collagens in the intervertebral disc. Collagen II comprises almost all of the total collagen in the nucleus pulposus, the amount of which decreases towards the outer structures so that it is absent or almost absent in the outer annulus fibrosus, while collagen I comprises almost all of the total collagen composition of the outer annulus fibrosus and decreases to absent or almost absent in the nucleus pulposus (Eyre & Muir 1977, Buckwalter 1995, Nerlich et al. 1998). Many reports indicate the presence of collagen IX in the intervertebral disc, even though Roberts et al. (1991) failed to immunolocalize it in the normal human disc (Ayad et al. 1982, Newall & Ayad 1995, Nerlich et al. 1998). Collagen IX has been found in all the compartments of the intervertebral disc, although it comprises about 2% of the total collagen or even less. Both short and long forms of collagen IX can be found, the short form predominating in the nucleus pulposus (Newall & Ayad 1995). By contrast, collagen XI has been found only in the nucleus pulposus, where it comprises about 3% of total collagen. Proteoglycans, primarily aggrecan, are a significant component of intervertebral discs accounting for a few percent of the dry weight of the annulus fibrosus, but about 50 percent of the nucleus pulposus. (See Buckwalter 1995.) 2.4. Disorders affecting cartilage collagens Numerous conditions that affect the components of cartilage have been characterized. The development and maintenance of cartilage can be affected at several stages in the life-span: the defects can already occur during embryogenesis, in the early steps of mesenchymal differentiation, or only after middle age. The mechanisms of the faulty processes are various. Transcription factors, growth factors, growth factor receptors, structural proteins or enzymes involved in their modification can be defective, or else the process can be due to inflammatory autoimmune disease, trauma or simply wear and tear. (See Horton & Hecht 1993, Mundlos & Olsen 1997a, Mundlos & Olsen 1997b, Kuivaniemi et al. 1997, Cremer et al. 1998.) Only disorders affecting cartilage collagens are discussed in the following. In the case of a cartilage collagen defect, the symptoms may appear in all or some of the tissues in which the collagens are expressed. Probably the most common symptom is destruction of the hyaline cartilage of joints. The development of bony structures such as the spine, long bones and facial bones is often defective due to the disruption of endochondral ossification. Interestingly, the eye and ear can be severely affected: high myopia, retinal detachments and hearing deficits are usual manifestations of cartilage collagen defects. (See Spranger et al. 1994, Mundlos & Olsen 1997b.) 25 2.4.1. Achondrogenesis type II-hypochondrogenesis (ACGII-HCG) Initially, achondrogenesis type II (Langer-Saldino type) and hypochondrogenesis were considered two separate disorders (Langer et al. 1969, Saldino 1971, Maroteaux et al. 1983), but after individuals with an intermediate phenotype had been characterized they often came to be regarded as different degrees of severity of the same disorder (Borochowitz et al. 1986). Infants with ACGII-HCG (OMIM #200610) die perinatally or within the first weeks of life. The disorder is characterized by a short, barrel-shaped trunk, very short extremities, a large head, a soft cranium, a flat face and hydropic appearance. Radiographically, the affected infants show varying degrees of underossification of the axial skeleton. Histological and electron microscopic examinations reveal hypercellular epiphyseal cartilage with poorly organized or absent growth plate and diminished extracellular matrix that contains thick, irregular collagen fibrils together with large chondrocytes with a dilated rough endoplasmic reticulum. Biochemical studies of hyaline cartilage from ACGII-HCG infants have indicated abnormal and diminished collagen II, even its absence, and the presence of collagen I. (Eyre et al. 1986, Godfrey et al. 1988, Godfrey & Hollister 1988, see also Horton & Hecht 1993, Spranger et al. 1994.) As suggested by earlier biochemical data, the genetic defect causing ACGII-HCG was found in the COL2A1 gene (Vissing et al. 1989). Over ten mutations causing ACGIIHCG have been reported, and all of them involve the replacement of glycine by a bulkier amino acid in the triple helical region of the α1(II) chain. The disorder is caused by heterozygous mutations, and naturally, because of the severity of the symptoms, the cases are usually sporadic. (See Horton & Hecht 1993, Kuivaniemi et al. 1997.) 2.4.2. Spondyloepiphyseal dysplasia (SED) Spondyloepiphyseal dysplasia (SED, OMIM #183900) is characterized by a short trunk, short extremities, a barrel-shaped chest, kyphosis and lordosis, severe myopia, and often retinal detachments, cleft palate and clubfoot. Affected infants usually survive. Radiographs show defects in ossification of the spine and primarily proximal extremities. (See Horton & Hecht 1993.) Histological studies show defects resembling those in ACGII-HCG, and biochemical examination indicates abnormalities in collagen II (Yang et al. 1980, Murray et al. 1989). SED refers to a heterogeneous group of disorders that affect the spine and epiphyses, and as the symptoms resemble those of ACGII-HCG, SED can be considered to represent the mild end of the spectrum comprising ACGIIHCG and SED phenotypes (see Spranger et al. 1994). Most cases of SED show autosomal dominant inheritance, but an autosomal recessive form of inheritance has also been suggested in some cases (Harrod et al. 1984, see also Horton & Hecht 1993). Lee et al. (1989) identified a deletion of an entire exon in the COL2A1 gene, leading to a lack of 36 amino acids in the triple helical region of the α1(II) chain, and subsequently numerous mutations, including insertions, mutations causing aberrant RNA splicing, glycine mutations and a cystein for arginine substitution, have been characterized (see Vikkula et al. 1994, Kuivaniemi et al. 1997). However, 26 some investigations have excluded the COL2A1 gene as a locus for SED in certain families, indicating that there must also be some other locus or loci for the disorder (Wordsworth et al. 1988, Anderson et al. 1990). 2.4.3. Kniest dysplasia Patients with Kniest dysplasia (OMIM #156550) have a round face, midfacial hypoplasia, prominent eyes and high myopia. Cleft palate, hearing loss and retinal detachment are also frequent manifestations of the disorder. The trunk and extremities are shortened and the joints are enlarged and exhibit restricted mobility. Numerous abnormal characteristics are seen in radiographic examinations. There is generally flattening of the vertebral bodies, the long bones are shortened and of a dumbbell shape due to expanded metaphyses, while the epiphyses are irregular and fragmented, the joint spaces are narrow, and there is generalized osteopenia in their ends. Kniest dysplasia is usually more severe than SED and is lethal in some cases. (Chen et al. 1980, see also Horton & Hecht 1993, Spranger et al. 1994.) Histologically, the cartilage is soft and vacuolar, and electron microscopy shows abnormally thin and irregular collagen fibrils in the matrix and dilated rough endoplasmic reticulum (Horton & Rimoin 1979, Poole et al. 1988, Gilbert-Barnes et al. 1996.) Kniest dysplasia is an autosomal dominant disorder. More than ten heterozygous mutations in the COL2A1 gene have been reported to date, including that in the patient originally described by Dr. Kniest in 1952. All except two of them lead to whole or partial exon deletions, and all but one are clustered in the N terminal half of the molecule, thus indicating that the cause of Kniest dysplasia lies in short in-frame deletions in this particular region of the collagen II molecule. (Spranger et al. 1997, Fernandes et al. 1998, see also Kuivaniemi et al. 1997.) Recent studies have shown that a significant fraction of the defective collagen II molecules are secreted and incorporated in cartilage collagen fibrils. Furthermore, it has been hypothesized that the normal α1(II) chains would form a loop and thus allow in-register triple helix formation in both directions from the deletion site. Moreover, due to the susceptibility of the loop to protease cleavage, this could also account for the degenerate vacuolar appearance of the cartilage matrix in patients with Kniest dysplasia. (Weis et al. 1998, Fernandes et al. 1998.) 2.4.4. Stickler and Marshall syndromes Stickler syndrome (OMIM #108300), originally called hereditary progressive arthroophthalmopathy, is an autosomal dominantly inherited disorder. Patients have high myopia, vitreoretinal degeneration and frequently retinal detachments and cataracts. Midfacial hypoplasia and micrognathia are often accompanied by cleft palate or a lesser degree of clefting, and sensorineural hearing defect is common. The skeletal manifestations include juvenile progressive arthropathy, irregularity of the vertebral bodies and hypermobile joints. Skeletal growth is usually normal. Mild epiphyseal 27 dysplasia and overtubulation of long bones are seen in radiological examination. (Stickler et al. 1965, Stickler & Pugh 1967, see also Herrmann et al. 1975, Temple 1989, Snead & Yates 1999.) In addition, an increased prevalence of mitral valve prolapse has been reported (Liberfarb & Goldblatt 1986), but this was not supported in the echocardiographic studies of over 100 patients (see Snead & Yates 1999). Marshall syndrome (OMIM #154780) is also an autosomal dominantly inherited disorder, and closely resembles Stickler syndrome. The ocular, facial and auditory features are much alike, but patients with Marshall syndrome are usually short in stature and have intracranial ossifications, abnormal frontal sinuses and thickened calvaria. In addition, Dr. Marshall originally reported some kind of hypohidrotic ectodermal dysplasia associated with the other symptoms, but it is thought nowadays that ectodermal dysplasia is not involved in the syndrome. (Marshall 1958, O’Donnell et al. 1976, Aymé & Preus 1984, Stratton et al. 1991, Shanske et al. 1997, Warman et al. 1998.) Numerous new cases of Stickler or Marshall syndrome have been reported since the original kindreds, and these have broadened the range of characteristics, so that it is now clear that there is clinical heterogeneity within the disease phenotypes, especially in Stickler syndrome (Herrmann et al. 1975, Zlotogora et al. 1992). The similar features of Stickler and Marshall syndromes have led to a clinical debate as to whether the syndromes are two distinct entities or just different manifestations of a single entity (Baraitser 1982, Winter et al. 1983, Aymé & Preus 1984, Stratton et al. 1991, Shanske et al. 1997). Furthermore, the diagnosis of Marshall syndrome has aroused some debate (Shanske et al. 1998, Warman et al. 1998). Another autosomal dominantly inherited syndrome with ocular manifestations is Wagner syndrome, or hyaloideoretinal degeneration of Wagner (OMIM #143200). This was originally characterized by myopia, cataract, vitreoretinal degeneration and often retinal detachment, but no manifestations in non-ocular tissues. There are some reports of Stickler-like non-ocular symptoms in Wagner syndrome, however, leading to a suggestion that the two could represent the same disorder. (See Liberfarb et al. 1979, Horton & Hecht 1993.) Linkage studies have shown that the COL2A1 gene is a locus for Stickler syndrome (Francomano et al. 1987, Knowlton et al. 1989). Altogether nine mutations have been reported to date, all of them leading to premature termination of translation (Ahmad et al. 1991, Brown et al. 1992, Ahmad et al. 1993, Ritvaniemi et al. 1993, Brown et al. 1995a, Ahmad et al. 1995, Williams et al. 1996). The same gene was also found to be a locus for Wagner syndrome in one family (Körkkö et al. 1993), even though Wagner syndrome, together with erosive vitreoretinopathy, is normally linked to 5q13-q14 (Brown et al. 1995b). The COL2A1 gene has also been excluded in several families with Stickler syndrome (Knowlton et al. 1989, Vintiner et al. 1991, Bonaventure et al. 1992), and Snead et al. (1994) have suggested that Stickler families with congenital vitreous anomaly (Stickler syndrome type 1) have linkage to the COL2A1 gene, while in those with congenitally defective vitreous gel architecture but no congenital vitreous anomaly (Stickler syndrome type 2) linkage is excluded. Subsequently, Richards et al. (1996) demonstrated linkage to the COL11A1 gene in a family with Stickler syndrome type 2, and traced it to a missense mutation converting glycine to valine in the N terminal part of the triple helix of the α1(XI) chain. In addition, Wilkin et al. (1998) have suggested still another locus for Stickler syndrome apart from the genes coding for collagens II and XI. 28 It was also hypothesized that Marshall syndrome was caused by mutations in the COL11A1 gene (van Steensel et al. 1997). A splicing mutation that led to a deletion of 18 amino acids in the C terminal half of the α1(XI) triple helical region was found to be associated with the phenotype (Griffith et al. 1998). 2.4.5. Otospondylomegaepiphyseal dysplasia (OSMED), WeissenbacherZweymüller syndrome (WZS) and non-ocular Stickler-like syndrome Otospondylomegaepiphyseal dysplasia (OSMED, OMIM #215150) is an autosomal recessive chondrodysplasia characterized by sensorineural deafness, spondyloepiphyseal dysplasia with large epiphyses, disproportionate shortness, midfacial hypoplasia and often micrognathia and cleft palate, but no ocular manifestations (Giedion et al. 1982, Kääriäinen et al. 1993, van Steensel et al. 1997). Electron microscopic examination of cartilage shows disorganized matrix with extremely thick collagen fibres that consist of aggregated thinner fibrils (van Steensel et al. 1997). Weissenbacher-Zweymüller syndrome (WZS, OMIM #277610)) is highly similar to OSMED and is also thought to be an autosomal recessive disorder. One characteristic of WZS is its favourable progression during childhood. (Cortina et al. 1977, Chemke et al. 1992.) Vikkula et al. (1995) demonstrated linkage to the COL11A2 gene in a family with OSMED, and also identified a homozygous mutation in the gene. The mutation led to a substitution of arginine for glycine in the N terminal half of the triple helical region of the collagen XI molecule. The original patient with WZS described by Drs. Weissenbacher and Zweymüller in 1964 was also found to have a mutation in the COL11A2 gene. The mutation converted a glycine to glutamate in the C terminal end of the triple helix, and, surprisingly, was heterozygous. (Pihlajamaa et al. 1998b.) Furthermore, a kindred with an autosomal dominant disorder resembling Stickler syndrome but without eye involvement was linked to chromosome 6 near to the COL11A2 gene (Brunner et al. 1994), and subsequently Vikkula et al. (1995) reported of a heterozygous mutation in the kindred causing exon skipping in the COL11A2 mRNA and thus deletion of 18 amino acids near the C terminal end of the triple helical region in the α2(XI) chain. A mutation causing deletion of 9 amino acids in the middle of the triple helical region was described in another family with a Stickler-like syndrome without eye involvement (Sirko-Osadsa et al. 1998). The nomenclature for the chondrodysplasias caused by mutations in the COL11A2 gene was established before the common molecular background for the disorders had been discovered, and thus the terminology is confusing, with various names applying to the same disorders. Recent findings have led to a suggestion for a new nomenclature for these disorders. The term heterozygous OSMED was introduced to include the former WZS and non-ocular Stickler-like syndrome, while homozygous OSMED is recommended for recessive OSMED. (Pihlajamaa et al. 1998b, Spranger 1998.) 29 2.4.6. Multiple epiphyseal dysplasia (MED) The typical finding in patients with multiple epiphyseal dysplasia (MED; OMIM #132400), an autosomal dominantly inherited disorder, is prominent and frequently painful joints with restricted mobility. This usually appears in early childhood. The disorder affects multiple joints rather than being generalized, and it leads to precocious osteoarthritis. The patients have a waddling gait and may have short and stubby hands. Stature is normal or moderately short with normal proportions. Radiographic examination shows typically small, irregular epiphyses. (Barrie et al. 1958, Hoefnagel et al. 1967, Spranger et al. 1974, van Mourik et al. 1998a.) The severity of symptoms varies considerably, and some patients with radiological evidence of MED do not have any complaints (van Mourik et al. 1998a). MED is often divided into two subgroups, the mild Ribbing type and the severe Fairbank type (see International Working Group on Constitutional Diseases of Bone 1998). Because of the wide phenotypic spectrum of MED, not all patients with the disorder can be classified into either the Ribbing or the Fairbank type, and it has been suggested that these terms should be abandoned (van Mourik et al. 1998a, Haga et al. 1998). The Ribbing type has also been reported to be recessive, but molecular genetic studies on such families suggest germline mosaicism as an explanation (Deere et al. 1995, Loughlin et al. 1998). Pseudoachondroplasia (PSACH, OMIM #177170) is an autosomal dominant disorder that resembles MED but is more severe, causing disproportionate dwarfism and ligamentous laxity. Radiographs show abnormalities in the epiphyses, metaphyses and spine. (See Horton & Hecht 1993.) Genetic linkage of both MED and PSACH to the pericentromeric region of chromosome 19 has been demonstrated (Hecht et al. 1993, Briggs et al. 1993, Oehlmann et al. 1994). This is where the gene for cartilage oligomeric matrix protein (COMP), a pentameric calcium binding glycoprotein of the extracellular matrix, is located (Newton et al. 1994). A large number of mutations causing either MED or PSACH have been reported in the COMP gene (Briggs et al. 1995, Hecht et al. 1995, Ikegawa et al. 1998), but it has also been excluded in a MED family, where linkage was demonstrated to a region of chromosome 1 containing the COL9A2 gene (Briggs et al. 1994). Muragaki et al. (1996) identified a splicing mutation of exon 3 in the COL9A2 gene, leading to a lack of 12 amino acids in the COL3 domain of the α2(IX) chain. Recently, another mutation in collagen IX was reported in a family with MED, causing a splicing defect of exon 3 with a similar consequence to that reported earlier but applying to the COL9A3 gene. (Paassilta et al. 1999a.) Similar dilatations of the rough endoplasmic reticulum in chondrocytes can be seen in MED and PSACH (Stanescu et al. 1982, Stanescu et al. 1993). These were studied further in a PSACH patient who was shown to have a mutation in the COMP gene. The dilatations contained aggregates consisting of at least COMP and collagen IX, suggesting a common pathogenic mechanism for MED and PSACH. (Maddox et al. 1997b.) No dilatation of the rough endoplasmic reticulum was seen in patients with MED caused by the COL9A2 mutation, however (van Mourik et al. 1998b). 30 2.4.7. Osteoarthritis (OA) Osteoarthritis, or osteoarthrosis (OA), is the most common articular disorder and is characterized by joint pain and tenderness, stiffness, crepitus and limitation of motion. Radiographs typically show joint-space narrowing, osteophytes, subchondral bone sclerosis and subchondral cyst formation. In severe cases deformity of the bone ends is also seen. OA is classified into primary (idiopathic) or secondary subsets; in a primary case there is no known predisposing factor, while in a secondary case such a factor is known, e.g. trauma, infection, a mechanical factor, some other joint disorder or a metabolic disease. Further classification divides OA into localized, in which only certain joints are affected, and generalized subsets. Even though it is often considered only an inevitable consequence of ageing, female sex, obesity, occupational load and heavy sports exertion are risk factors for it. (See Moskowitz 1989, Altman 1995, Creamer & Hochberg 1997.) The suggestion of genetic factors underlying OA in certain families was made several decades ago (Stecher 1941, Stecher et al. 1953, Kellgren et al. 1963). In 1989, Palotie et al. demonstrated a linkage to the COL2A1 gene in a family with primary OA. Knowlton et al. (1990) made a similar finding in a family with precocious OA and associated mild chondrodysplasia, and Ala-Kokko et al. (1990) subsequently demonstrated a mutation in this family. The mutation converted arginine to cysteine, an amino acid not normally found in the triple helical domains of collagens, in the middle of the triple helix of the collagen II molecule. Altogether five families with this same mutation have been reported to date, and three of them have been shown to have a common ancestor (see Bleasel et al. 1995, Kuivaniemi et al. 1997, Bleasel et al. 1998). In addition, a mutation converting arginine to cysteine at position 75 near the N terminus of the triple helix has been reported in three families with OA associated with mild SED (see Bleasel et al. 1995, Bleasel et al. 1996). 2.5. Animal models for disorders of the cartilage collagens In order to fully understand the mechanisms of a cartilage disorder, histological and molecular studies are essential. Human cartilage specimens for such studies are difficult to obtain, because that would require a surgical operation, and perhaps more importantly, spare cartilage is rarely available, at least in large amounts. Furthermore, it is well known that chondrocytes dedifferentiate in cell culture (Grundmann et al. 1980). Animal models, often mice, are thus used for cartilage disorders. The phenotype is either a natural variant of the species or is generated by the scientist by introducing mutagenic agents into the animal, or more elegantly, by manipulating the genome by modern techniques that allow targeted mutation, inactivation or specific expression of virtually any gene. Large amounts of cartilage specimens can be obtained from animal models, and disorders can also be studied in vivo. 31 2.5.1. Collagen II Several approaches have been used for studying collagen II defects in mice. Two transgenic mouse lines with deletions in the triple helical domain have been generated, and two with glycine substitutions. The phenotypes caused by these mutations are usually perinatally lethal chondrodysplasias characterized by dwarfism, short snout, cleft palate, disorganized growth plates and reduced ossification. The collagen fibrils are disorganized and reduced in amount. (Vandenberg et al. 1991, Garofalo et al. 1991, Metsäranta et al. 1992, Maddox et al. 1997a.) A phenotype resembling this has also been produced in a mouse line with disproportionate micromelia (Dmm) generated by irradiation (Brown et al. 1981). These mice have a deletion in the region encoding the C propeptide of procollagen II, which leads to a substitution of one amino acid for two (Pace et al. 1997). Garofalo et al. (1993) overexpressed collagen II. The mice died at birth, but they did not exhibit cleft palate, abnormal craniofacial features, or other skeletal deformities, except for a slight reduction in the length of the long bones. Electron microscopy of the cartilage showed abnormally thick, extensively branched fibrils, which led to the suggestion that the imbalance in cartilage components caused by the overexpression of collagen II disrupted the mechanism that controls the diameter of the fibrils. On the other hand, total inactivation of the Col2a1 gene generated by S.-W. Li et al. (1995) in mice led to severe perinatally lethal chondrodysplasia. This mouse model shed some light on the role of cartilage in skeletal development by showing that collagen II is essential for the development of endochondral bone and epiphyseal cartilage but not that of many other skeletal structures such as membranous and periosteal bone. 2.5.2. Collagen IX Three mouse lines with defective collagen IX have been generated. Mice expressing a truncated α1(IX) chain, which lack part of the COL2 domain, the entire NC3 domain and part of the COL3 domain, were shown to develop osteoarthritis, which was mostly obvious in the knee joints. Ones with a higher level of transgene expression also developed mild chondrodysplasia with mild proportionate dwarfism and a slight ossification defect in the spine. Abnormally thin collagen fibrils were seen in electron microscopy. (Nakata et al. 1993.) Furthermore, long-term follow-up of the mice revealed accelerated intervertebral disc degeneration, which occasionally led to herniation and osteophyte formation (Kimura et al. 1996). Fässler et al. (1994) generated a mouse line lacking the α1(IX) chain. The mice showed no detectable abnormalities at birth, but later developed a severe progressive degenerative joint disease resembling human OA, which was most prominent in the knee joints. The fibril morphology of the cartilage was nevertheless visually identical in the homozygous and control mice. Absence of the α1(IX) chain was shown to lead to absence of the α2(IX) and α3(IX) chains as well, even though they were transcribed. Thus this mouse line exhibited functional inactivation of the entire collagen IX. These findings lead to a suggestion that collagen IX is essential for the integrity of the cartilage matrix, but not for skeletal development. (Hagg et al. 1997.) 32 Transgenic mice expressing multiple copies of a minigene coding for the NC4 domain of collagen IX have also been created. This overexpression of the NC4 domain induced osteoarthritis analogous to human OA. (Haimes et al. 1995.) 2.5.3. Collagen XI One mouse model for collagen XI disorders has been reported. Mice with autosomal recessive chondrodysplasia (cho) have disproportionately short limbs with wide, flared metaphyses and abnormal facial features consisting of a short snout, short mandible, protruding tongue and cleft palate. They have soft tracheal cartilage rings, which is probably the cause of their perinatal death. Microscopy showed disorganized growth plates and abnormally thick collagen fibrils. (Seegmiller et al. 1971.) Linkage studies mapped the cho locus to the region containing the Col11a1 gene, and a frame shift mutation causing premature translation termination was identified. The mutation thus leads to absence of the α1(XI) chain. The finding indicates the importance of this chain for skeletal morphogenesis and, more specifically, for the formation of proper collagen fibrils in cartilage. (Li Y et al. 1995.) 2.6. Intervertebral disc disease Degenerative changes in the intervertebral discs begin early in childhood. The degeneration occurs in all parts of the discs, but the nucleus pulposus undergoes the most extensive changes. The annulus fibrosus generally expands at the expense of the nucleus pulposus, the number of viable cells in the disc decreases and the water concentration also decreases. The amounts of proteoglycans decrease, and fragmentation of the aggregating proteoglycans can be detected. The pathomechanism of these changes is not known, but one potential cause could be a decline in nutrition due to the increasing volume of the disc during growth and a simultaneous age-related decrease in the arteries supplying nutrients and removing waste. Even if disc degeneration is an inevitable consequence of ageing, it can vary greatly in rate and extent within the same person and between individuals. (See Buckwalter 1995.) The degeneration impairs the structural integrity of the disc tissue and increases the probability of functional deficiency and disc herniation. In intervertebral disc herniation part of the nucleus pulposus extrudes through the annulus fibrosus. The extruded material may cause mechanical compression or chemical irritation to the adjacent nerve root and lead to sciatica, i.e. radiating pain in the dermatome of the root. (See Hasue 1993, Alaranta & Poussa 1994.) Herniation of the lumbar discs and sciatica, also called lumbar disc syndrome, is a common disorder affecting the Finnish population with a prevalence of about 5% (Heliövaara et al. 1987). Many environmental risk factors for intervertebral disc disease have been proposed, including hard physical work, driving motor vehicles and smoking (see Heliövaara 1989), but genetic predisposition to advanced disc degeneration and intervertebral disc disease has also been suggested, and it has even been 33 claimed that this may be the primary factor (Varlotta et al. 1991, Scapinelli 1993, Battié et al. 1995, Sambrook et al. 1999). In addition, polymorphisms in the vitamin D receptor gene have been associated with intervertebral disc degeneration (Videman et al. 1998). 2.6.1. Cmd mice Mice that are homozygous for cartilage matrix deficiency (cmd) have short limbs, trunk, tail and snout, cleft palate and hearing impairment, and they die at birth, probably of respiratory failure (Rittenhouse et al. 1978, Yoo et al. 1991). The mice were found to lack aggrecan (Kimata et al. 1981), and a deletion causing premature translation termination in the gene coding for aggrecan has been identified (Watanabe et al. 1994). Despite the original understanding that the heterozygous mice are normal, Watanabe et al. (1997) demonstrated that they show dwarfism and spinal misalignment at the age of one year. They exhibited deformation of the vertebral bodies, advanced disc degeneration and disc herniations, but no changes in other cartilaginous tissues. This finding supports results obtained with mice expressing a truncated α1(IX) chain, indicating that mutations in the genes coding for cartilage matrix protein can cause intervertebral disc disease. Mice with hereditary kyphoscoliosis (ky) also develop advanced intervertebral disc degeneration, but these changes are secondary to a neuromuscular disorder that leads to atrophy of the muscles supporting the spine (Mason & Palfrey 1984, Bridges et al. 1992). 2.7. Mutation detection methods Knowing the genetic defect behind a disease provides a basis for understanding the disease and treating it. The detection of new, previously unknown mutations in sequences of a candidate gene requires an appropriate method. Sequencing is a thorough method, but if the sequences to be searched span thousands or tens of thousands of base pairs, the procedure turns out to be expensive and excessively laborious. A large number of methods for mutation detection, most of them based on PCR, have been introduced to make it more efficient with regard to costs, time and work. The methods usually take advantage either of the change in electrophoretic mobility produced by the mutation or of recognition and cleavage of the mismatched site in a heteroduplex comprising a mutant and a wild strand. (See Cotton 1989, Cotton 1993, Eng & Vijg 1997, Nollau & Wagener 1997.) 2.7.1. Commonly used methods based on electrophoresis Single-strand conformation polymorphism (SSCP) is based on the fact that singlestranded DNA has a defined secondary structure under certain conditions. This secondary structure changes if the sequence is altered, and this is detected in the form of mobility 34 shifts on a polyacrylamide gel. (Orita et al. 1989a, Orita et al. 1989b.) Band visualization has to be performed with radiolabelling or silver staining, as ethidium bromide, which is widely used to stain double-stranded DNA, does not stain single-stranded DNA efficiently. The advantage of SSCP is the simplicity of the procedure, but its sensitivity, which is best with fragments less than 200 bp, is only 60-95%. (See Cotton 1993, Eng & Vijg 1997.) The melting properties of double-stranded DNA depend on the sequence of the DNA fragment. This phenomenon is utilized in denaturing gradient gel electrophoresis (DGGE) by electrophoresing DNA fragments on a polyacrylamide gel under increasing denaturing conditions. Thus sequence variations alter the melting and mobility of the mutant fragment as compared with a control fragment. (Fischer & Lerman 1983, see also Myers et al. 1987.) The original method was able to detect sequence variations only in the low melting domains of the fragment, i.e. sequences with a low melting temperature, giving a sensitivity of about 50%, but the addition of an artificial high melting GC-rich sequence (GC-clamp) to one end of the fragment using PCR primers converts the whole fragment to a low melting region and greatly improves the sensitivity (Sheffield et al. 1989). Fragments of up to 1 kb can be analyzed, but ones of 150-500 bp are usually most appropriate. The advantage of DGGE is its high sensitivity of almost 100%, but optimization of the melting properties of the fragment and electrophoresis conditions is laborious and time-consuming. (See Cotton 1989, Cotton 1993, Ganguly & Prockop 1995.) Heteroduplex analysis (HA or HET) is based on the different mobilities of homoduplexes and heteroduplexes on a non-denaturing polyacrylamide gel. Heteroduplexes, i.e. double-stranded DNA which contains one strand of the mutant type and one of the wild type, are formed by heat denaturation and subsequent reannealing of the two forms of DNA. (See Glavac & Dean 1995.) HA is a simple method that does not require optimizing, but its sensitivity is estimated to be about 80% (Cotton 1993). Many modifications of HA have been used to improve the sensitivity (see Glavac & Dean 1995). In conformation sensitive gel electrophoresis (CSGE), mildly denaturing agents are used to enhance the conformational changes in the heteroduplexes. Sensitivity is also improved by using 1,4-bis(acryloyl)piperazine (BAP) instead of the commonly used Bis as a crosslinker in the polyacrylamide gels. Even though CSGE is a simple method, it has been reported to detect most mutations in fragments of 200-800 bp. (Ganguly et al. 1993, Ganguly & Prockop 1995.) 2.7.2. Commonly used methods based on cleavage of a mismatch A mismatch in a heteroduplex creates a short region of single-stranded DNA, which can be detected by an enzyme or a chemical that cleaves single-stranded DNA. In enzyme mismatch cleavage (EMC), bacteriophage T4 endonuclease VII and/or T7 endonuclease I is used to cleave the site of the mismatch. EMC can be used for fragments of up to 1.5 kb. The method is relatively sensitive, but some unspecific background can also be observed. (Youil et al. 1995, Mashal et al.1995.) Chemical mismatch cleavage (CMC) is a two- 35 phase procedure in which the DNA is first treated with hydroxylamine and osmium tetroxide, which react with mismatched cytosines and thymines, respectively, and piperidine is then added to cleave the modified mismatched base. Fragments up to 2 kb can be screened with a sensitivity of 100%, but the toxic reagents are a major drawback. (Cotton et al. 1988, see also Cotton 1993, Nollau & Wagener 1997.) 2.7.3. Other methods Carbodiimide (CDI) is a bulky reagent that reacts with thymine and guanine residues. The CDI modification procedure for mutation detection is based on the observation that CDI reacts more rapidly with unpaired bases than with paired ones. Electrophoresis, nuclease cleavage, immuno electron microscopy and primer extension have been used to detect the modified bases (Novack et al 1986, Thomas et al. 1988, Ganguly et al. 1989, Ganguly & Prockop 1990). In the primer extension method, which is probably the most practical of these, CDI blocks primer extension and shorter products can be identified by electrophoresis. DNA fragments of up to 1 kb can be used, and the location of the mutation can be estimated to an accuracy of about 15 bp. The advantage of the immuno electron microscopy method is that a mutation can be detected in a heteroduplex of several kilobases. (See Cotton 1993.) Cleavase fragment length polymorphism (CFLP) is based on the secondary structure changes that a sequence variation generates. Cleavase I endonuclease cleaves the singlestranded DNA at the bifurcated end of a double-stranded region, and thus generates DNA fragments of different lengths depending on the sequences. (Lyamichev et al 1993, see also Nollau & Wagener 1997.) A mismatch binding protein MutS, which is a component of the Eschericia coli DNA repair system, can also be used to detect mutations in heteroduplexes. Various methods, including mobility shift assays, biotinylated MutS, solid-phase assay with immobilized MutS and an optical biosensor have been used to detect MutS binding (Lishanski et al. 1994, Wagner et al. 1995, Geschwind et al. 1996, Gotoh et al 1997). Advantage has also been taken of the protective feature of the MutS protein against endonucleases for detection purposes (Ellis et al. 1994). The protein truncation test (PTT) is specific to mutations causing premature translation termination. A T7 promoter and a eucaryotic translation initiation sequence are added to the fragment of interest by PCR, after which the fragment is transcribed and translated. A premature translation termination codon results in shortening of the translation product, which can be detected in electrophoresis. (Roest et al. 1993, see also Nollau & Wagener 1997.) The most recent methods for mutation detection require special equipment and computerized analysis. Denaturing high-performance liquid chromatography (DHPLC) is based on the high resolution separation of heteroduplexes from homoduplexes under controlled partially denaturing conditions. The method is highly sensitive and the commercially available procedure (Transgenomic WAVETM System) is fully automated. (Hayward-Lester et al. 1995, Liu et al. 1997/98, O’Donovan et al. 1998.) Oligonucleotide microarray (DNA chip) technology will be a promising method for mutation detection in 36 the future. It is based on hybridization of the sample to a large number of immobilized oligonucleotide microarrays fabricated by advanced manufacturing processes. The method has an enormous capacity, and many applications have been demonstrated for it. (See Marshall & Hodgson 1998, Ramsay 1998, Hacia 1999.) 3. Outlines of the present research Collagen II is the main collagen in cartilage, and mutations in the COL2A1 gene coding for the collagen II homotrimer are known to cause a spectrum of chondrodysplasias ranging from lethal ACGII-HCG to early-onset OA associated with mild chondrodysplasia. In general, a certain phenotype predicts a certain type of mutation in the COL2A1 gene. Kniest dysplasia, for example, is usually caused by a mutation leading to a short in-frame deletion in the N terminal half of the triple helix, while a glycine substitution at the C terminal end of the triple helix often leads to ACGII-HCG. Collagens IX and XI are minor cartilage collagens which are also expressed in the intervertebral disc, ocular vitreous body and tectorial membrane of the inner ear. At the time when this research project was initiated, only one mutation had been reported in collagen IX. This was in the COL9A2 gene and led to MED. Four mutations in collagen XI had been reported, two of which were in the COL11A1 gene, one leading to Stickler syndrome and the other to Marshall syndrome, while two of them were in the COL11A2 gene, one leading to OSMED and the other to Stickler-like syndrome without ocular involvement. Based on the collagen II studies it was hypothesized that mutations in collagens IX and XI would also cause a spectrum of phenotypes. The object of this work was therefore to increase our knowledge of the role of collagens IX and XI in disorders affecting cartilaginous tissues. The specific aims were: 1. to improve the sensitivity of conformation sensitive gel electrophoresis (CSGE), 2. to characterize the genomic structure of the human COL11A1 gene and to set up the CSGE method for the gene, 3. to clarify the relation between the Marshall and Stickler syndromes by analyzing the COL11A1 and COL2A1 genes in patients with Marshall and Stickler syndromes for mutations by CSGE and comparing the two syndromes on the basis of the genetic and clinical data, and 4. to analyze the COL9A2 gene in patients with intervertebral disc disease for mutations by CSGE. 4. Materials and methods The materials and methods are described in detail in the original papers I-III. 4.1. Subjects and clinical examination methods (I-III) Altogether 30 patients with a suspected diagnosis of Marshall or Stickler syndrome were referred to us from several departments of genetics, ophthalmology and surgery in Finland, Israel, the Netherlands, Norway, Poland and the USA. The clinical diagnosis was established by a clinician familiar with this morphology and experienced with these disorders. Informed consent was obtained from the patients. 157 unrelated Finnish patients with sciatica, defined as unilateral pain of duration over one month radiating from the back to below the knee, and the family members of four of the patients were referred to us from Department of Physical Medicine and Rehabilitation and the Department of Internal Medicine at Oulu University Hospital. The patients were evaluated clinically and radiologically by experienced clinicians. Altogether 174 Finnish controls consisting of 101 asymptomatic subjects, 54 patients with OA and 19 patients with various chondrodysplasias but no history of sciatica were included in the study. The OA patients were referred to us from the Department of Surgery at Kuopio University Hospital. The radiological examinations of the patients with sciatica were performed by magnetic resonance imaging (MRI) in 156 cases and by computed tomography (CT) in one case. The MRI scans, obtained with a 1.5-T imaging system (Signa, General Electric, Milwaukee, Wisconsin), consisted of sagittal images with a TR/TE of 4000/95 ms and axial images with a TR/TE of 640/14 ms. The CT images (Hi Speed Advantage, GE Medical Systems, Milwaukee, Wisconsin) consisted of scans through the L2-L3 interspace to the L5-S1 interspace. The radiographs were read by two neuroradiologists blinded to the results of the clinical and genetic examination and the clinical histories of the patients. The following radiological findings were considered indications of intervertebral disc disease: (1) disc extrusion, (2) any herniation at two or more levels, (3) endplate degeneration at one or more levels in patients under 30 years of age, at two or more levels in patients aged 30-50 years or at four or more levels in patients over 50 39 years, or (4) bulging and/or protrusion at four or more levels (Jensen et al. 1994, Weishaupt et al. 1998). Genomic DNA was extracted from the venous blood or cultured fibroblasts by standard protocols and used for the analyses. 4.2. Characterization of the COL11A1 gene (II) To characterize the genomic structure of the COL11A1 gene and obtain intronic sequences of the gene required for the CSGE analysis, screenings for genomic clones were ordered from Genome Systems, Inc. PCR probes were designed based on the published cDNA sequences (Bernard et al. 1988) and the sequences obtained here by sequencing intronic PCR products amplified with exon specific primers. PCR probes for the subsequent screenings were designed based on sequences defined from clones obtained in previous screenings. The probes were from 5’UTR, exon/intron 2, intron 4, intron4/intron5, exons 27/28, intron 28/intron 29, intron 52/intron 53 and 3’UTR. Altogether five clones, one P1, two PACs, and two BACs were found, each containing a part of the gene. The P1 clone was transferred from the Escherichia coli NS3529 strain to the NS3516 strain, which gives a higher yield, via transduction according to the instructions provided by Genome Systems. The plasmid DNA preparations were performed using a standard plasmid isolation protocol recommended by the manufacturer. The genomic organization and intronic sequences were defined, either directly from the clones or from PCR products amplified from the clones, using an automated sequencer (ABI PRISM 377 Sequencer and dRhodamine or BigDye Termination Cycle Sequencing Kit with AmpliTaq DNA Polymerase, FS, Perkin-Elmer; Expand Long Template PCR System, Boehringer Mannheim). For regions that were not included in the clones, the PCR amplifications for sequencing were performed from genomic DNA. The sequencing primers were designed based on the cDNA sequences or sequences defined in this work. The sizes of the introns up to about 1.5 kb were defined by sequencing, and the sizes of the other introns were defined by PCR amplification (Expand Long Template PCR System, Boehringer Mannheim). Unspecific amplification was ruled out either by sequencing the ends of the PCR products or by using two different sets of PCR primers for each intron. 4.3. CSGE (I-III) The PCR products for CSGE analysis were amplified from genomic DNA. The primers were designed to amplify the target sequence and about 50 bp of both the 5’ and 3’ flanking sequences. The primers were designed initially to generate PCR products of 200-800 bp, as suggested in the previous reports (Ganguly et al. 1993, Ganguly & Prockop 1995), but during experiments designed to improve the method the size 40 requirement of the PCR product was changed to 200-450 bp. The PCR amplifications were typically carried out in a reaction volume of 40 µl containing 50-100 ng of genomic DNA, 200µM of each dNTP, 0.25 µM of each primer and 1 unit of Taq polymerase (AmpliTaq Gold, Perkin-Elmer). The cycling conditions consisted of initial denaturation for 10 min at 95°C followed by 30-35 cycles of 95°C for 20-40 sec, 54-60°C for 30-40 sec and 72°C for 20-40 sec, followed by a final extension at 72°C for 4-10 min. Heteroduplexes were generated at the end of the PCR cycling by denaturing the PCR products at 95-98°C for 3-5 min and reannealing at 68°C for 30 min. An aliquot of 50100 ng was mixed with loading buffer (10 x stock solution of 30% glycerol - 0.25% bromphenol blue - 0.25% xylene cyanol FF) and loaded onto a CSGE gel. CSGE analysis was performed with a 1 mm gel in a standard DNA sequencing apparatus with 33 x 40 or 37.5 x 45 cm glass plates. The initial gel composition was 10% of a 1:99 ratio of 1,4-bis(acrolyol)piperazine (BAP; Fluka) to acrylamide (Intermountain Scientific), 10% ethylene glycol (Sigma), 15% formamide (Gibco), 0.1% ammonium persulphate (APS; U.S. Biochemicals) and 0.07% N,N,N’,N’-tetramethylethylenediamine (TEMED; Sigma) in 0.5 xTTE buffer (44mM Tris - 14.5 mM taurine - 0.1 mM EDTA, pH 9.0), according to the previously published protocol, and the gel was electrophoresed at 400 V for 16 hours (Ganguly et al. 1993, Ganguly & Prockop 1995). In the course of experimentation to improve the method, the gel composition was changed to contain 1215% BAP-acrylamide, and the electrophoresis was performed at 40 W for 6 to 8.5 hours depending on the size of the glass plates. After the electrophoresis, the gel was stained with ethidiumbromide (1 µg/ml) on a glass plate and a relevant piece was cut out, transferred onto a UV transilluminator and photographed with a high quality chargecoupled device (CCD) camera (Fotodyne or UVP). 4.4. Screening of the COL11A1 and COL2A1 genes of patients with Marshall and Stickler syndromes for mutations by CSGE (II) PCR primers suitable for CSGE analysis of the COL11A1 gene were designed based on the intronic sequences defined in this work. The entire coding region of the gene, excluding exons 2 and 4, was amplified in 67 fragments. The CSGE analysis for the COL2A1 gene was performed by the procedure set up by Körkkö et al. (submitted), according to the protocol described in section 4.3. After amplification, the PCR products were analyzed on an agarose gel to check the quantity and quality of the products and to reveal any large deletions or insertions. The CSGE analysis was then performed using the improved conditions described in paper I. The samples showing heteroduplexes in CSGE were subjected to automated sequencing (ABI PRISM 377 Sequencer and dRhodamine or BigDye Termination Cycle Sequencing Kit with AmpliTaq DNA Polymerase, FS, Perkin-Elmer) using one of the PCR primers as the sequencing primer. The PCR products had been treated prior to this with exonuclease I and shrimp alkaline phosphatase to remove residual PCR primers and nucleotides (Werle et al. 1994, Hanke & Wink 1994). The physicians of the patients found to have a mutation were asked to provide complete clinical data to substantiate the diagnosis of either Marshall or Stickler 41 syndrome and to perform a genotypic-phenotypic comparison. All available family members of such patients were also analyzed for the presence of the mutation. 4.5. RT-PCR (II) RT-PCR analysis was performed on a patient, who had a sequence variation at the +3 position in intron 50 of the COL11A1 gene to study the effect of the variation in splicing. Total RNA was extracted from cultured skin fibroblasts (RNeasy Midi Kit, Qiagen) and used as a template for first strand synthesis (Superscript Preamplification System, Gibco BRL), which was performed with the oligo(T) primer under the conditions suggested by the manufacturer for transcripts with a high GC content. The subsequent PCR amplifications of the illegitimate transcripts were performed using α1(XI) cDNA specific primers, and the products obtained were sequenced. 4.6. Screening of patients with sciatica for mutations in the COL9A2 gene (III) The patients with sciatica were screened for mutations in the COL9A2 gene using PCR primers suitable for CSGE analysis designed on the basis of previously defined sequences (Pihlajamaa et al. 1998a). Initially, a subset of patients with sciatica were screened for mutations in the COL9A2 gene by the method described in section 4.3. After a unique sequence variation in exon 19 had been found in one of these patients, exon 19 was amplified in the samples from all the other patients and controls using the PCR primers 5’-TGG ATC TCA GTT TCC CTA CCT G (-92 to -71 in intron 18) and 5’-CAA GAG GTG GTG ATT GAG CAA GAG C (+99 to +75 in intron 19). The PCR products were analyzed for sequence variation by CSGE and sequencing (ABI PRISM 377 Sequencer and dRhodamine or BigDye Termination Cycle Sequencing Kit with AmpliTaq DNA Polymerase, FS, Perkin-Elmer), and some of the PCR products were cloned prior to sequencing (T7 Sequencing Kit, Pharmacia). The family members of four patients who were found to have the sequence variation in exon 19 were evaluated clinically and radiologically, and genetic analysis for the presence of the mutation was performed to study the co-segregation of the genotype with the phenotype. 4.7. Statistical analysis (III) The statistical analysis to evaluate the significance of the sequence variation was performed by Harald H. H. Göring at the Department of Genetics and Development of Columbia University, New York, USA, using the ILINK program of the FASTLINK computer package. 42 According to the clinical and radiological examinations, pedigree members of the four families who tested positive for the disease in either the clinical or the radiological test were coded as affected, and those testing negative in both tests were coded as unaffected. Individuals who were not examined or examined only clinically or radiologically and found to be normal were coded as being of unknown phenotypic status. In addition, artificial pedigrees were created from the case-control data to enable linkage and linkage disequilibrium analyses to be performed jointly on the pedigrees and singletons by coding two case or control individuals as the parents of a hypothetical offspring of unknown phenotype (Kainulainen et al. 1999). 5. Results 5.1. Optimization of CSGE (I) To test and improve the sensitivity of CSGE for mutation detection, genes coding for collagen α chains were selected for examination. Collagen genes are challenging targets for mutation detection because they are complex, consisting of large numbers of exons, and the sequences are repetitive and GC-rich due to the numerous glycine and proline residues. Previously known sequence variations in the COL1A1, COL1A2, COL2A1, COL3A1, COL9A1 and COL9A2 genes were used as references in the optimization. In order to improve the sensitivity of CSGE, the lengths of the PCR products used for the analyses, the electrophoresis conditions and the acrylamide concentrations in the gel were altered to test the sensitivity under different conditions. 5.1.1. Improved conditions for mutation detection by CSGE (I) The original report on CSGE suggested that the procedure could be applied to PCR products of size 200-800 bp (Ganguly et al. 1993). However, sequence variations were detected less frequently in PCR products of 500-800 bp than in shorter products, and a common polymorphism in exon 25 of the COL1A2 gene (Constantinou et al. 1990) was not detected in a PCR product of 755 bp whereas it was clearly detected when the region containing the polymorphism was amplified to generate a PCR product of less than 300 bp (Fig. 1 in paper I). Some other PCR products of over 500 bp were also found to contain polymorphisms using shorter PCR products (data not shown). This finding led to a suggestion that only PCR products of up to 450 bp should be used to ensure the sensitivity of the method. The electrophoretic conditions were altered to test whether the detection of poorly detectable sequence variations could be improved and to speed up the procedure. The electrophoresis was performed with 40 W for 6 hours instead of a overnight run with 400 V. The separation of heteroduplexes on the gel was improved under the altered electrophoretic conditions in several cases (see Fig. 2A and 2B in paper I), and a specific 44 test with 48 heteroduplexes detected previously under the original conditions did not indicate any disappearance of these (data not shown). Furthermore, a few previously undetected sequence variations became detectable with the new electrophoretic conditions (data not shown). In addition, the BAP-acrylamide concentration in the gel was increased from 10% to 15% to see if it would improve the separation of the heteroduplex bands in CSGE. With the higher concentration of the polymer the running time was increased to 8.5 hours. This improved the detection of a single base polymorphism in intron 11 of the COL1A1 gene, which was previously poorly detected (Fig. 2C and 2D in paper I). To test these alterations further, over 200 single base pair changes that had previously been detected using 10% polyacrylamide gels and electrophoretic conditions of 400 V overnight or 40 W for 6 hours were analyzed using 15% polyacrylamide gels with running conditions of 40 W for 8.5 hours. The separation was found to be better under the new conditions. 5.1.2. Testing the sensitivity and specificity of CSGE Altogether 76 previously identified single base changes detected by nucleotide sequencing of the COL1A1 gene (Körkkö et al. 1998), DGGE analysis of the COL1A1 and COL2A1 genes (Ritvaniemi et al. 1993, Ritvaniemi et al. 1995, Körkkö et al. 1997), or sequencing of the cDNAs for α chains of collagens I and III (see Ganguly et al. 1993) were used to test the sensitivity of CSGE. All the changes except one, which was not consistently revealed, were detected using the improved CSGE procedure (Table 1 in paper I). The specificity of the method was tested by sequencing 223 PCR products that generated heteroduplexes in CSGE. In addition, over 200 PCR products that did not generate heteroduplexes in CSGE were sequenced as controls. All the products that generated a heteroduplex yielded at least one sequence variation, while no sequence variations were found in the controls (Table 2 in paper I). These results indicate that CSGE does not generate false-positive or false-negative results to any significant extent. A sequence variation in the PCR product resulted in a unique heteroduplex band that was usually readily distinguishable from other possible sequence variations or their combinations in the product (Fig. 6 in paper I). Only rarely were heteroduplex bands observed that looked similar but were generated by different sequence variations in the PCR product (data not shown). 5.2. Characterization of the human COL11A1 gene (II) All three genes coding for collagen IX α chains have been characterized (Pihlajamaa et al. 1998a, Paassilta et al. 1999b) as have the COL11A2 and COL2A1 genes, which code for the α2(XI) and α3(XI) chains of collagen IX (Ala-Kokko et al. 1995, Vuoristo et al. 1995). For the COL11A1 gene, which codes for the α1(XI) chain, only the cDNA sequence and a few exon-intron boundaries had previously been known (Bernard et al. 45 1988, Zhidkova et al. 1995). To complete the information on the genomic structures of the genes coding for collagen XI and to set up a mutation screening method for this gene, the human COL11A1 gene was characterized here. 5.2.1. Characterization of clones for the COL11A1 gene Altogether five clones for the human COL11A1 gene, one P1, two PAC and two BAC clones, were obtained from the screenings ordered from Genome Systems, Inc. The locations of the introns and the intronic sequences flanking the exons were defined by sequencing with exon-specific primers and primers designed on the basis of the intronic sequences defined here. The exons were numbered in a manner corresponding to the numbering of exons in the COL11A2 gene (Vuoristo et al. 1995). The P1 clone (address DMPC-HFF#1-140(B10)) was found to contain the sequences from intron 4 to intron 29, both of the PAC clones (addresses PAC-84:8A and PAC-154-1M) contained the sequences from intron 4 to intron 54, one of the BAC clones (address 170O21) contained the sequences from intron 4 to intron 63, and the other BAC clone (address BACH-86N5) contained the sequences from an undefined distance from the 5’-end of the gene to intron 1 (Fig. 1 in paper II). 5.2.2. Genomic structure of the human COL11A1 gene Although PCR probes for screening of the P1, PAC and BAC libraries were used from exon/intron 2, intron 4, and 3’-UTR, no clones containing the sequences from intron 1 to intron 4 or sequences in the 3’-direction of intron 63 were found. Most of the structure and sequences of these regions were defined by sequencing PCR products amplified from genomic DNA, but several attempts to amplify introns 1 and 4 failed and thus their size remained undefined. The gene was found to consist of 68 exons (Fig. 1 in paper II, Table 1 in paper II), which were numbered from 1 to 67, using the numbers 6A and 6B for the sixth and seventh exons (previously called IIA and IIB), because they are alternatively spliced and do not exist in the same mRNA (Zhidkova et al. 1995). The exon numbers 9-15 previously used by Bernard et al. (1988) correspond to exons 16-22 in this numbering. The locations of the exon-intron boundaries in the major triple helical region of the COL11A1 gene were exactly the same as those in the COL11A2 gene (Table 1 in paper II, Vuoristo et al 1995). The sizes of the introns were defined by sequencing or PCR amplification. The size of the gene, excluding introns 1 and 4, was about 160 kb (Table 1 in paper II). The intronic sequences flanking the exons were sequenced and over 50 kb of new sequences were defined for the gene. The sequences were submitted to GenBank (accession numbers AF101079-AF101112). 46 5.2.3. Resequencing of the coding region Resequencing of the coding region indicated some differences relative to the published cDNA sequence (Bernard et al. 1988). No cysteinyl residue was found in the triple helical region, and the amino acid sequence at positions 413-416, calculated from the first glycine of the main triple helical domain, was Lys-Asp-Gly-Leu instead of the previously reported Arg-Met-Gly-Cys. In addition, the amino acid at position 690 was methionine instead of tryptophan, an amino acid rarely found in collagen triple helices. These sequences were defined from 150 alleles. 5.3. Identification of mutations in the COL11A1 and COL2A1 genes in patients with Marshall or Stickler syndrome (II) The CSGE method was set up for the COL11A1 gene based on the sequences defined here and a corresponding analysis for the COL2A1 gene was performed by the procedure set up by Körkkö et al. (submitted). A group of 30 patients who had been referred to us with a suspected diagnosis of Marshall or Stickler syndrome were screened for mutations in these two genes. Altogether 23 mutations were identified, fifteen in the COL11A1 gene and eight in the COL2A1 gene. 5.3.1. Identification of mutations in the COL11A1 and COL2A1 genes by CSGE All exons and exon boundaries except those of exons 2 and 4 of the COL11A1 gene were amplified by PCR and heteroduplexes were generated. The PCR products were analyzed on an agarose gel to check their quantity and quality and reveal any large insertions or deletions. The agarose gel analysis of the products for exon 53 suggested a heterozygous deletion of about 150 bp in one patient. The sequencing indicated a 162 bp deletion that contained 85 bp of intron 52, exon 53, and 23 bp of intron 53. CSGE analysis was performed on the rest of the patients, and several unique heteroduplexes were observed. Sequencing identified ten mutations that altered the splicing consensus sequences, two small in-frame deletions in the coding sequences, and two glycine substitutions (Table 2 in paper II). A similar procedure was performed to analyze the COL2A1 gene in the patients for whom no mutations were found in the COL11A1 gene, and altogether eight novel mutations were found by CSGE analysis and sequencing. Six of these caused a frameshift leading to premature translation termination codons, and two of them altered the splicing consensus sequences (Table 2 in paper II). In the familial cases the mutation was found to cosegregate with the phenotype (data not shown). All except two of the mutations altering the splicing consensus sequences affected the conventional AG-dinucleotide at the acceptor splice site or the GT-dinucleotide at the donor splice site. One of the remaining two was an A to C change and the other was an 47 insertion of T at position +3 in intron 50 of the COL11A1 gene. To study the effect of the A to C change on splicing, RT-PCR analysis was performed for illegitimate mRNA transcripts extracted from the patient’s cultured skin fibroblasts. Two PCR products were obtained, one corresponding to the wild type cDNA sequence and one lacking the sequences for exon 50. No RNA was available from the patient with the insertion, but DNA was obtained from the parents, who were unaffected, and analyzed for the presence of the insertion. Neither parent had the insertion (data not shown). In the familial cases those family members who were available were examined for the presence of the mutation and for clinical symptoms. The mutation was found to cosegregate with the phenotype (data not shown). 5.3.2. Genotypic-phenotypic comparison All the COL11A1 mutations were found in the region coding for the major triple-helical domain. Ten out of fifteen mutations altered the splicing consensus sequences for 54 bp exons, and one genomic deletion led to the loss of a 54 bp exon. Eight of these mutations affected exons 48-54, four of them exon 50. The analysis also identified two in-frame deletions of 18 bp and 9 bp in exons 36 and 52, respectively. In addition, two glycine substitution mutations were found (Fig. 1, table 2 in paper II). Fig. 1. Schematic drawing of the COL11A1 transcript and the locations of the mutations. The major triple helix is left blank and all the other regions are shaded. The areas corresponding to the exons are separated by the horizontal lanes and are drawn to scale. The locations of all the mutations found in the COL11A1 gene are marked with the identification number of the corresponding patient (Table 2 in paper II). The mutations marked above the drawing are splicing mutations in the C terminal half of the molecule (1 to 8 and 10) and a genomic deletion including a 54 bp exon (9). Those marked below the drawing are glycine substitution mutations (12 and 15), small in-frame deletions (13 and 14), and a splicing mutation in the N terminal end of the triple helix (11). 48 The patients who were found to have a mutation, were evaluated clinically, with particular emphasis on the major findings characteristic of the Stickler and Marshall syndromes, in order to evaluate the phenotypic consequences of the COL11A1 and COL2A1 mutations. Particular attention was paid to the characteristics reported to differ between these syndromes. It has been suggested that the syndromes differ in that patients with Marshall syndrome are more often of short stature, deaf and have abnormalities in cranial ossification and more pronounced dysmorphic features, including a retracted midface with flat nasal bridge, short nose, anteverted nostrils and a long philtrum. Furthermore, it has been suggested that retinal detachment occurs less frequently in patients with Marshall syndrome. (O’Donnell et al. 1976, Aymé & Preuss 1984, Stratton et al. 1997.) In general, the phenotypes in the COL11A1 and COL2A1 genes resembled each other (Table 1, table 3 in paper II). The clinical findings in the patients who had a mutation in either of the genes typically consisted of high myopia, midfacial hypoplasia, palatal defects and retro/micrognathia. There were some major differences, however. The vast majority of patients with COL11A1 mutations had moderate to severe hearing impairment that was congenital or detected in early childhood, whereas the patients with COL2A1 mutations had normal hearing or minor hearing loss that usually developed later in life. The ocular findings were generally more severe in the patients with COL2A1 mutations than in those with COL11A1 mutations, in that almost all of the former had vitreoretinal degeneration and retinal detachment. Furthermore, cataracts were more common in patients with COL2A1 mutations than in the patients with COL11A1 mutations. Slight differences were also seen in stature and facial characteristics (Table 3 in paper II). Midfacial hypoplasia, a short nose and a flat nasal bridge were more clearly pronounced in Marshall syndrome, and did not disappear when the child grew older (Fig. 2 in paper II). Radiographic skeletal evaluations could be performed only on a few patients, as radiographs were available only for those with skeletal complaints. Osteoarthritic changes seemed to be more common in the cases with COL2A1 mutations, but many of the patients were too young to be evaluated for such changes. Cranial radiographs were available only for six cases with COL11A1 mutations and two with COL2A1 mutations. None of the latter had cranial abnormalities, but four of the former group had abnormalities such as abnormal frontal sinuses, intracranial ossifications and/or a thickened calvarium. The patients with COL11A1 and COL2A1 mutations could be divided into three groups based on the phenotype and mutational type (Table 1). The first group had a splicing mutation of a 54 bp exon or a genomic deletion of a 54 bp exon in the COL11A1 gene region coding for the C terminal half of the α1(XI) molecule, and their characteristics resembled those reported in Marshall syndrome (Aymé & Preuss 1984, Shanske et al. 1997, Griffith et al. 1998). The second group had other mutations in the COL11A1 gene and phenotypes overlapping both the Marshall and Stickler syndromes, while the third group had a mutation in the COL2A1 gene and a phenotype that closely resembled the classical Stickler syndrome (Stickler et al. 1965, Stickler & Pugh 1967, Herrmann et al. 1975). 49 Table 1. Summary of the clinical data. Findings COL11A1 mutations patients 1-10 a patients 11-15 COL2A1 mutations b patients 16-23 moderate to severe hearing loss 10/10 4/5 0c/7 ocular findings high myopia retinal detachment vitreoretinal degeneration cataract 10/10 1/10 3/9 4/10 4/5 2/5 3/5 3/5 8/8 6/8 5/7 5/7 facial features short nose anteverted nares midface hypoplasia flat nasal bridge palate defect micro/retrognathia long philtrum epicanthus hypertelorism lowered auricles 10/10 10/10 10/10 10/10 8/10 8/10 7/9 7/9 6/10 4/8 4/5 4/5 4/5 4/5 4/5 3/5 3/5 2/5 0/4 0/3 5/7 3/6 7/7 6/7 8/8 4/6 4/6 3/5 2/7 1/4 stature short tall 6/10 0/10 3/5 1/5 2/7 2/7 cranial findings abnormal frontal sinuses intracranial ossifications thick calvarium 2/3 1/3 2/4 1/1 1/2 1/2 0/2 0/2 0/2 dental abnormalities 1/9 0/2 1/3 a b c splicing mutation of a 54 bp exon or genomic deletion causing a loss of 54 bp in exons coding for the C terminal half of the α1(XI) molecule other mutations in the COL11A1 gene 3 of the cases had a minor hearing deficit 50 5.4. Identification of an allele of the COL9A2 gene associated with intervertebral disc disease (III) 5.4.1. Identification of a tryptophan for glutamine/arginine substitution in the COL9A2 gene The CSGE method for the COL9A2 gene was set up based on the published sequences (Pihlajamaa et al. 1998a), and ten patients with intervertebral disc disease were initially analyzed for mutations in the gene. A unique CSGE pattern was found in the PCR product for exon 19 in one of the patients (Fig. 1 in paper III), and sequencing identified a heterozygous substitution of Trp (TGG) for Gln (CAG) at amino acid position 326. Analysis of exon 19 in all 157 patients with intervertebral disc disease indicated that six of them had the Trp substitution. The analysis was also performed on the 174 controls, who consisted of 101 asymptomatic individuals, 54 with OA and 19 with various chondrodysplasias but no history of sciatica. None of the controls had the Trp substitution. Sequencing of exon 19 also indicated that Arg (CGG) was found relatively often at position 326, suggesting that the Trp allele had arisen from the Arg allele by a single base substitution (Fig. 2 in paper III). The frequency of the Arg substitution was about the same in the patient group and all of the control groups, indicating that it was a neutral polymorphism (Table 1 in paper III). 5.4.2. Co-inheritance of the Trp allele and intervertebral disc disease To study whether the Trp allele is co-inherited with intervertebral disc disease, the families of four patients with this allele were included in the study. The two other families were not available for examination. The families were evaluated clinically and by CT (family A) or MRI (families B, C and D), and analyzed for the presence of the Trp allele. As stated in the Materials and methods section, the individuals were considered affected if they had either clinical or radiological evidence of the disease, or both. All the family members who had inherited the allele had intervertebral disc disease (Fig. 2). 5.4.3. Statistical analysis Linkage analysis and linkage disequilibrium analysis were performed to evaluate the statistical evidence for a connection between the Trp allele in the COL9A2 gene and intervertebral disc disease. Since the aetiology of the disease is multifactorial (Heliövaara 1989), a high phenocopy rate was specified. In the selected model the disease locus accounts for 10% of cases, in other words, 90% of patients with intervertebral disc disease are affected for reasons unrelated to this particular disease locus. A fully penetrant dominant disease model was chosen for the analysis and the disease prevalence 51 Fig. 2. The pedigrees of the four families studied. The right half of each symbol indicates the clinical findings, and the left half the radiological findings. The symbol is black when the finding is positive, and a dot indicates that the family member was examined and found to be normal. A blank symbol indicates that the individual was not examined. The proband is marked with an arrow. The family members with the Trp allele are indicated by (+), and the members who did not have the allele are indicated by (-). 52 was set at 4.8%, which is the estimated frequency of sciatica in Finland (Heliövaara et al. 1987). Artificial pedigrees were created from the case-control data to enable a linkage and linkage disequilibrium analysis to be carried out jointly on the pedigrees and singletons (Kainulainen et al. 1999). Linkage disequilibrium analysis gave a lod score of 4.5 at a recombination fraction of 0.12. Subsequent linkage disequilibrium given the presence of linkage was analyzed, and an additional lod score of 7.1 was obtained. The joint lod score was therefore 11.6 (Table 2 in paper III). A similar analysis was performed with the recombination fraction fixed at 0.0 (Table 3 in paper III). The lod scores were lower, but that does not necessarily contradict the hypothesis that the Trp allele itself caused the disease. The explanation is rather the inaccuracy of the model used. For common diseases such as intervertebral disc disease it is practically impossible to specify a model with 100% accuracy, and thus reduced lod scores and overestimated recombination fractions are obtained as a result of model inaccuracies. (Clerget-Darpoux et al. 1986, Risch & Giuffra 1992, see also Terwilliger & Ott 1994.) To examine the extent to which the results were dependent on the assumed disease model, individual parameters of the model were varied keeping the predicted population prevalence unchanged at 4.8%. The linkage and linkage disequilibrium lod scores remained high for a dominant model when the proportion of cases explained by the disease locus was varied and when high but incomplete penetrance was used (Table 2 in paper III). 5.4.4. Scanning the entire COL9A2 gene for mutations in patients with the Trp allele To determine whether there were other sequence variations in the COL9A2 gene among the patients whose disease was linked to this gene, all the exons and exon boundaries were analyzed by CSGE. The analysis did not identify any other possible disease causing mutation of coding sequences or RNA splice sites, but it did identify two additional neutral polymorphisms, an A to G change at the third nucleotide in the codon for proline at nucleotide 9 in exon 21 and a G to A change at nucleotide +17 in intron 30. These were analyzed in 90 and 286 individuals, respectively, but were not found in any individuals other than those with the Trp allele. 6. Discussion 6.1. Detection of mutations by CSGE The detection of unknown mutations in one or more candidate genes is a challenging task, especially with large, complex genes. Sequencing would be a thorough method, but it is too laborious and expensive. Numerous PCR-based screening methods, each having typical advantages and disadvantages, are available for mutation detection (see Cotton 1989, Cotton 1993, Eng & Vijg 1997, Nollau & Wagener 1997), but typical drawbacks are the radioactive or toxic chemicals required for the procedure and problems of sensitivity or specificity. Screening a large number of samples in complex genes requires an easy, powerful method that maintains sensitivity in all sequence contexts but does not require separate optimization for different PCR products. In addition to being large in size and containing dozens of exons, collagen genes are problematic for mutation detection due to their repetitive sequences and high content of G and C residues. This is a consequence of the obligatory sequence for collagens, which consists of a glycine residue as every third amino acid, which is coded by a codon that always starts with two G residues, and has a high content of proline residues, which are coded by codons that always start with two C residues. CSGE is a relatively recent method that has many advantages, including nonradioactivity, a standard procedure for all fragments, large capacity and the use of standard equipment. Furthermore, it has been reported to have relatively high sensitivity, detecting 60 out of 63 single base pair changes in PCR fragments of 200-800 bp. (Ganguly et al. 1993, Ganguly & Prockop 1995.) No reports on its sensitivity have been published, however, since the initial one by Ganguly et al. (1993). To study CSGE further, modifications of the procedure were developed and tested with large number of known sequence variations, including the three changes that were not detected in the initial report. The procedure was improved by using shorter PCR products, a higher polymer concentration in the gel and more powerful electrophoretic conditions. To test the sensitivity of the improved method, 76 previously identified sequence variations were tested and all the changes except one, which was not consistently identified, were detected. Furthermore, 223 samples with unique CSGE patterns, along with over 200 PCR products with only homoduplexes on the gel, were 54 sequenced to test the specificity of the procedure. All of the samples with heteroduplexes on CSGE and none of the samples with only homoduplexes had sequence variations. This indicates that the sensitivity and specificity of CSGE under the improved conditions are close to 100%. In addition to the high sensitivity and specificity, CSGE proved to be a simple and practical method. No special optimization is required, which allows different fragments to be analyzed simultaneously. The generation of heteroduplexes, which can be added to the end of the PCR program, is the only special treatment required for the samples. Standard sequencing apparatus is used for the electrophoresis, and the loading of multiple samples of different sizes into the same lane provides for a high capacity. Unique CSGE patterns are usually seen for the different sequence variations on the gel. This makes it easy to avoid sequencing the same neutral polymorphisms in all the samples carrying it, and thus reduces the cost of the analysis and the work required. Although CSGE proved to be a highly sensitive and specific method, it has the same drawbacks as the other PCR-based procedures that make use of the formation of heteroduplexes. The alleles with a deletion or some other sequence variation at the PCR primer binding site of the fragment to be analyzed may not be amplified and thus will not be detected by CSGE, while insertions between the PCR primer sites may lengthen the fragment to such an extent that the allele is not amplified. Furthermore, equal amplification of both a normal and mutant allele cannot be ensured, and thus unequal amplification due to a low amount of the mutant allele in the PCR reaction, or its absence, can cause false negatives in the analysis. In addition, as the formation of heteroduplexes is based on the presence of two alleles with different sequences at the site of the mutation, the mutation will remain undetected if it is present in both alleles, as in the case of a homozygous mutation in a recessive disease. This can be overcome by mixing the patient sample with a control sample. 6.2. Genomic structure of the human COL11A1 gene Characterization of the human COL11A1 gene in P1, PAC and BAC clones and in genomic DNA indicated that the gene consists of 68 exons and spans at least 160 kb. The sizes for introns 1 and 4 remained undefined because no clones containing these sequences were found and attempts to amplify them by PCR failed. The exon-intron organization of the major triple helical region of the COL11A1 gene was identical to that of the COL11A2 gene, indicating a common evolution for these genes differing from that of the genes for the major fibrillar collagens, which have different numbers and sizes of exons (Vuorio & de Crombrugghe 1990, Vuoristo et al. 1995). The COL11A1 and COL11A2 genes are completely different in size, however, the former being over 160 kb and the latter only 28 kb. The COL11A1 gene resembles COL5A1 in size, the latter being about 150 kb excluding the first intron, the size of which has not been defined (Takahara et al. 1995). These two genes are also identical in the exon-intron organization of the major triple helical region, except for one area in which there are two exons of 54 bp in the COL11A1 gene corresponding to one exon of 108 bp in the COL5A1 gene. Furthermore, the exon-intron organization of the C propeptides of these genes is 55 identical. These findings support the previous assumption of a close relation between the α chains of collagens V and XI. The size of intron 1 of the COL5A1 gene has been thought to be at least 600 kb, and that of intron 4 is 26 kb (Takahara et al. 1995). This suggests that the failure to amplify the sequences of introns 1 and 4 of the COL11A1 gene by PCR was caused by their large size. 6.3. COL11A1 and COL2A1 gene mutations in patients with Marshall or Stickler syndrome Two mutations in the COL11A1 gene have been identified, one in Marshall syndrome and the other in Stickler syndrome (Richards et al. 1996, Griffith et al. 1998). The COL11A1 gene is the only locus for Marshall syndrome identified thus far, but Stickler syndrome has also been shown previously to be caused by mutations leading to a premature translation termination in the COL2A1 gene (see Kuivaniemi et al. 1997). A clinical debate on the identity and diagnosis of Marshall and Stickler syndromes has been going on for decades (O’Donnell et al. 1976, Baraitser 1982, Winter et al. 1983, Aymé & Preus 1984, Stratton et al. 1991, Shanske et al. 1997, Shanske et al. 1998, Warman et al. 1998). To study the issue by a genetic approach, the COL11A1 and COL2A1 genes in patients with Marshall or Stickler syndrome were screened for mutations by CSGE. Altogether 23 mutations were identified, fifteen in the COL11A1 gene and eight in the COL2A1 gene. The majority of those in the COL11A1 gene altered the splicing consensus sequences, all of them affecting the 54 bp exons, as in the previously reported case (Griffith et al. 1998). Furthermore, one patient had a genomic deletion resulting in the loss of a 54 bp exon. Ten out of these eleven mutations were in a region spanning exons 38 to 54 of the gene. Although more than one third of the exons in this region are 90 or 108 bp in size, no splicing mutations or deletions affecting them were found. The only splicing mutation in the N terminal part of the α1(XI) triple helical region caused a very different phenotype from the other splicing mutations, one in which only severe ocular symptoms and shortness occurred, with no hearing deficit or facial features other than the high arched palate typical of the Stickler and Marshall syndromes. Six of the COL2A1 mutations resulted in a premature translation termination codon, and two altered the splicing consensus sequences. Fairly good correlation has been observed between the mutation type in the COL2A1 gene and the phenotype it causes (see Kuivaniemi et al. 1997). The two patients who had a splicing mutation had features typical of Stickler syndrome, with no signs of more severe Kniest dysplasia or SED, which are known to be consequences of splicing mutations leading to in-frame deletions in the COL2A1 gene. It is therefore likely that the mutations in the splicing consensus sequences of these patients lead to cryptic splice sites, and thus to premature translation termination codons, as was also reported in the original kindred described by Dr. Stickler (Williams et al. 1996). The finding that mutations in the COL11A1 and COL2A1 genes lead to similar phenotypes is not surprising. Types II and XI are both fibril-forming collagens and form components of the same fibril in cartilage. Furthermore, mutations in the COL11A2 gene, which codes for the α2(XI) chain, have been reported to cause homozygous and 56 heterozygous OSMED, which has features similar to the Stickler and Marshall syndromes (see Spranger 1998). The phenotypes caused by COL11A2 mutations nervertheless lack ocular involvement, because the α2(V) chain rather than the α2(XI) chain is expressed in the vitreous body (Mayne et al. 1993). Also, the correlation of the mutational types with the severity of the phenotypes they cause fits well with the amounts of these collagen types in the fibrils. Mutations leading to defective collagen molecules are known to cause more severe phenotypes than mutations causing haploinsufficiency (Kuivaniemi et al. 1997). In the cases described here, the mutations leading to a premature translation termination codon in a quantitatively more significant molecule in the fibrils generated a similar phenotype to the mutations causing expression of defective molecules of a quantitatively less significant fibril component. The present results indicate that patients with a COL11A1 mutation, especially those who had a splicing mutation or genomic deletion of a 54 bp exon in the C terminal half of the α1(XI) molecule, had findings related to Marshall syndrome, while the patients with a COL2A1 mutation had a more classical Stickler phenotype. The genotypic-phenotypic correlation detected here supports the old clinical suspicion of two separate entities. Other mutations in the COL11A1 gene, however, resulted in phenotypes overlapping both the Marshall and Stickler syndromes, and it is these that possibly explain the conflicting reports as to whether Stickler and Marshall syndromes are separate entities or not. The clinical distinction between these phenotypes provides important information on the prognosis for the patient’s symptoms. Furthermore, if an analysis of the genetic defect causing the phenotype is desired, the clinical distinction helps in choosing the right gene for this analysis. The hearing deficit is probably the most outstanding feature distinguishing between the phenotypes caused by mutations in the COL11A1 and COL2A1 genes. Fourteen out of fifteen patients with a COL11A1 mutation had earlyonset hearing loss and required hearing aids, but the patients with a COL2A1 mutation had normal hearing or only a mild hearing defect. Furthermore, ocular involvement was less severe in the patients with COL11A1 mutations, although there were several exceptions. The classification of the ocular symptoms suggested by Snead et al. (1994) could not be performed, because the type of vitreal abnormality was not defined here. Another interesting means of distinction could be the evaluation of facial characteristics. The patients with Marshall syndrome were found to have more clearly pronounced midfacial hypoplasia, a short nose and a flat nasal bridge. These features did not disappear when the child grew older, as can be observed in individuals with Stickler syndrome (Temple 1989, H. Kääriäinen, personal communication). Cranial abnormalities including abnormal frontal sinuses, intracranial ossifications and/or a thickened calvarium have been described in Marshall syndrome (Marshall 1958, Aymé & Preuss 1984, O’Donnell et al. 1976, Griffith et al. 1998), and although cranial radiographs were available for only a third of the present patients, the findings supported the suggestion that a mutation in the COL11A1 gene may cause abnormalities in cranial ossification. An attractive explanation for this would be the presence of high levels of mRNA for the COL11A1 gene in the calvaria and brain but only low amounts of the mRNAs for the COL11A2 and COL2A1 genes, as observed by Lui et al. (1995). 57 6.4. The association of a COL9A2 allele with intervertebral disc disease Six out of 157 patients with intervertebral disc disease carried the Trp for Gln/Arg substitution in the central collagenous domain of the α2(IX) chain, while none of the 174 controls did so. Furthermore, the substitution co-segregated with the phenotype in the families studied. The statistical analyses provided extremely strong evidence that the Trp allele was associated with intervertebral disc disease. Even though the Trp allele of the COL9A2 gene was tightly linked to the phenotype, the results do not prove a direct causal role for it in the aetiology of the disease, as it is possible that some other gene in close proximity to the COL9A2 gene that is in linkage disequilibrium with the Trp allele is the true disease locus. A role for collagen IX mutations in intervertebral disc disease has nevertheless been suggested in experiments with transgenic mice, where long-term follow-up of the mice expressing a mutant Col9a1 gene showed intervertebral disc degeneration and herniations (Kimura et al. 1996). On the other hand, the only known disease-causing collagen IX mutations in humans lead to MED, which is characterized primarily by articular complaints. However, only two mutations in the genes coding for collagen IX that cause MED have been reported, one in the COL9A2 gene and one in the COL9A3 gene, and both lead to similar deletions of 12 amino acids at exactly same location in the COL3 domain of the molecule, suggesting the importance of this domain for the pathogenesis of MED (Muragaki et al. 1996, Paassilta et al. 1999a). This does not contradict the present results, as it is well known that different mutations in the same collagen gene may lead to very different phenotypes. A mutation in the COL2A1 gene, for example, may lead to a cartilage disorder without ocular involvement, while another mutation in the same gene leads to a disorder with only ocular manifestations (Ala-Kokko et al. 1990, Körkkö et al. 1993). Furthermore, a 9 bp deletion in the region coding for the COL1 domain of collagen IX that represents a neutral variant without any phenotypic consequences has been identified in the COL9A3 gene (Paassilta et al. 1999b). Thus it would not be surprising for a splicing mutation in the COL3 domain and a Trp substitution in the COL2 domain of the collagen IX molecule to lead to different phenotypes. The Trp substitution was the only putative disease-causing sequence variation in the COL9A2 gene among the patients whose phenotype was linked to the gene. Even though there might be another such mutation in an intron or in the promoter region of the gene, or alternatively, the Trp substitution or the presumably neutral polymorphisms detected in the gene might cause aberrant splicing, there are several arguments to suggest that the Trp substitution itself is the cause of the disease. Trp is rarely found in the triple helices of collagens, and there are no Trp residues in any of the collagenous domains of human or mouse collagen IX (Muragaki et al. 1990, Perälä et al. 1993, Rokos et al. 1994, Perälä et al. 1994, Brewton et al. 1995), which suggests that it fits poorly into the collagen triple helix. Computerized molecular modelling of the sequence with Trp and the normal sequence indicated that the substitution alters the conformation of the helix (A. Fertala, unpublished data). It could also interfere with the covalent cross-link between the collagen II and collagen IX molecules. In the triple helical heterotrimer, the Lys residue in the α3(IX) chain that is involved in the cross-link is located only three amino acids away from the Trp substitution in the α2(XI) chain. 58 Studies on disc tissue from a patient carrying the Trp allele could perhaps reveal the mechanism by which the Trp causes the disease, but disc tissue from such patients is difficult to obtain for this purpose, at least in sufficient amounts. Preliminary results of in vitro studies performed with normal and Trp-carrying recombinant human collagen IX expressed in insect cells and recombinant human collagen II expressed in a transfected tumour cell line (HT1080) nevertheless indicate that collagen IX with the Trp allele has a higher affinity for collagen II than does normal collagen IX (S. Annunen, A. Fertala, D.J. Prockop, L. Ala-Kokko, unpublished data). The co-existence of the Trp allele and two other sequence variants indicated that the individuals with the Trp allele had inherited the same, relatively rare, ancestral haplotype. Interestingly, the same haplotype was also found in a Chinese immigrant, but he was not included in the series because an isolated Finnish population was thought to be a more accurate target for linkage disequilibrium analysis. This finding does indicate, however, that the haplotype with the Trp is not restricted to this genetically isolated Finnish population. Even though all the individuals with the Trp allele had intervertebral disc disease, there were some family members who had the disease but not the Trp allele. Intervertebral disc disease is common in the Finnish population, with a prevalence of 4.8%, and the Trp allele was found in about 4% of the patients, which leaves the remaining 96% of the cases to be explained by other genetic and environmental factors. Thus, it is not surprising that there are more than one aetiologies explaining the phenotype, even within one family. Although it is known that intervertebral disc disease has many environmental and anthropometric risk factors (see Heliövaara 1989), the present results indicate a role for genetic factors as well. This suggestion is supported by reports of familial intervertebral disc disease in the literature (Varlotta et al. 1991, Scapinelli 1993, Battié et al. 1995, Sambrook et al. 1999). 7. References Ahmad NN, Ala-Kokko L, Knowlton RG, Jimenez SA, Weaver EJ, Maguire JI, Tasman W & Prockop DJ (1991) Stop codon in the procollagen II gene (COL2A1) in a family with the Stickler syndrome (arthro-ophthalmopathy). Proc Natl Acad Sci USA 88: 6624-6627. Ahmad NN, McDonald-McGinn DM, Zackai EH, Knowlton RG, LaRossa D, Dimascio J & Prockop DJ (1993) A second mutation in the type II procollagen gene (COL2A1) causing Stickler syndrome (arthro-ophthalmopathy) is also a premature termination codon. Am J Hum Genet 52: 39-45. Ahmad NN, Dimascio J, Knowlton RG & Tasman WS (1995) Stickler syndrome. A mutation in the nonhelical 3’ end of type II procollagen gene. Arch Ophthalmol 113: 1454-1457. Ala-Kokko L, Baldwin CT, Moskowitz RW & Prockop DJ (1990) Single base mutation in the type II procollagen gene (COL2A1) as a cause of primary osteoarthritis associated with a mild chondrodysplasia. Proc Natl Acad Sci USA 87: 6565-6568. Ala-Kokko L, Kvist A-P, Metsäranta M, Kivirikko KI, de Chrombrugghe B, Prockop DJ & Vuorio E (1995) Conservation of the sizes of 53 introns and over 100 intronic sequences for the binding of common transcription factors in the human and mouse genes for type II collagen (COL2A1). Biochem J 308: 923-929. Ala-Kokko L & Prockop DJ (1990) Completion of the intron-exon structure of the gene for human type II procollagen (COL2A1): variations in the nucleotide sequences of the alleles from three chromosomes. Genomics 8: 454-460. Alaranta H & Poussa M (1994) Lanneselän sairaudet. In: Isomäki H, Leirisalo-Repo M & Hämäläinen M (eds) Reumataudit, 2nd ed. Duodecim, Helsinki, p 361-375. Altman RD (1995) The classification of osteoarthritis. J Rheumatol Suppl 43: 42-43. Anderson IJ, Tsipouras P, Scher C, Ramesar RS, Martell RW & Beighton P (1990) Spondyloepiphyseal dysplasia, mild autosomal dominant type is not due to primary defects of type II collagen. Am J Med Genet 37: 272-276. Ayad S, Abedin MZ, Weiss JB & Grundy SM (1982) Characterization of another short-chain disulphide-bonded collagen from cartilage, vitreous and intervertebral disc. FEBS Lett 139: 300-304. Ayad S & Weiss JB (1984) A new look at vitreous-humour collagen. Biochem J 218: 835-840. Aymé S & Preus M (1984) The Marshall and Stickler syndromes: objective rejection of lumping. J Med Genet 21: 34-38. Baraitser M (1982) Marshall/Stickler syndrome. J Med Genet 19: 139-140. Barrie H, Carter C & Sutcliffe J (1958) Multiple epiphyseal dysplasia. Br Med J 2: 133-137. Battié MC, Videman T, Gibbons LE, Fisher LD, Manninen H & Gill K (1995) 1995 Volvo Award in clinical sciences. Determinants of lumbar disc degeneration. A study relating lifetime exposures and magnetic resonance imaging findings in identical twins. Spine 20: 2601-2612. 60 Bengtsson E, Neame PJ, Heinegard D & Sommarin Y (1995) The primary structure of a basic leucine-rich repeat protein, PRELP, found in connective tissues. J Biol Chem 270: 2563925644. Bernard M, Yoshioka H, Rodriquez E, van der Rest M, Kimura T, Ninomiya Y, Olsen BR & Ramirez F (1988) Cloning and sequencing of pro-α1(XI) collagen cDNA demonstrates that type XI belongs to the fibrillar class of collagens and reveals that the expression of the gene is not restricted to cartilagenous tissue. J Biol Chem 263: 17159-17166. Birk DE, Fitch JM, Babiarz JP & Linsenmayer TF (1988) Collagen type I and type V are present in the same fibril in the avian corneal stroma. J Cell Biol 106: 999-1008. Bishop P (1996) The biochemical structure of mammalian vitreous. Eye 10: 664-670. Bleasel JF, Holderbaum D, Brancolini V, Moskowitz RW, Considine EL, Prockop DJ, Devoto M & Williams CJ (1998) Five families with arginine 519 - cysteine mutation in COL2A1: evidence for three distinct founders. Hum Mutat 12: 172-176. Bleasel JF, Holderbaum D, Haqqi TM & Moskowitz RW (1995) Clinical correlations of osteoarthritis associated with single base mutations in the type II procollagen gene. J Rheumatol Suppl 43: 34-36. Bleasel JF, Holderbaum D, Mallock V, Haqqi TM, Williams HJ & Moskowitz RW (1996) Hereditary osteoarthritis with mild spondyloepiphyseal dysplasia - are there ”hot spots” on COL2A1? J Rheumatol 23: 1594-1598. Bonaventure J, Philippe C, Plessis G, Vigneron J, Lasselin C, Maroteaux P & Gilgenkrantz S (1992) Linkage study in a large pedigree with Stickler syndrome: exclusion of COL2A1 as the mutant gene. Hum Genet 90: 164-168. Borochowitz Z, Ornoy A, Lachman R & Rimoin DL (1986) Achondrogenesis IIhypochondrogenesis: variability versus heterogeneity. Am J Med Genet 24: 273-288. Brewton RG & Mayne R (1992) Mammalian vitreous humor contains networks of hyaluronan molecules: electron microscopic analysis using the hyaluronan-binding region (G1) of aggrecan and link protein. Exp Cell Res 198: 237-249. Brewton RG & Mayne R (1994) Heterotypic type II, IX and XI fibrils: comparison of vitreous and cartilage forms. In: Yurchenco PD, Birk DE & Mecham RP (eds) Extracellular matrix assembly and structure. Academic Press, San Diego, p 129-170. Brewton RG, Wood BM, Ren ZX, Gong Y, Tiller GE, Warman ML, Lee B, Horton WA, Olsen BR, Baker JR & Mayne R (1995) Molecular cloning of the α3 chain of human type IX collagen: linkage of the gene COL9A3 to chromosome 20q13.3. Genomics 30: 329-336. Bridges LR, Coulton GR, Howard G, Moss J & Mason RM (1992) The neuromuscular basis of hereditary kyphoscoliosis in the mouse. Muscle Nerve 15: 172-179. Briggs MD, Choi H, Warman ML, Loughlin JA, Wordsworth P, Sykes BC, Irven CMM, Smith M, Wynne-Davies R, Lipson MH, Biesecker LG, Garber AP, Lachman R, Olsen BR, Rimoin DL & Cohn DH (1994) Genetic mapping of a locus for multiple epiphyseal dysplasia (EDM2) to a region of chromosome 1 containing a type IX collagen gene. Am J Hum Genet 55: 678-684. Briggs MD, Hoffman SMG, King LM, Olsen AS, Mohrenweiser H, Leroy JG, Mortier GR, Rimoin DL, Lachman RS, Gaines ES, Cekleniak JA, Knowlton RG & Cohn DH (1995) Pseudoachondroplasia and multiple epiphyseal dysplasia due to mutations in the cartilage oligomeric matrix protein gene. Nat Genet 10: 330-336. Briggs MD, Rasmussen IM, Weber JL, Yuen J, Reinker K, Garber AP, Rimoin DL & Cohn DH (1993) Genetic linkage of mild pseudoachondroplasia (PSACH) to markers in the pericentromeric region of chromosome 19. Genomics 18: 656-660. Brown DM, Graemiger RA, Hergersberg M, Schinzel A, Messmer EP, Niemeyer G, Schneeberger SA, Streb LM, Taylor CM, Kimura AE, Weingeist TA, Sheffield VC & Stone EM (1995b) Genetic linkage of Wagner disease and erosive vitreoretinopathy to chromosome 5q13-14. Arch Ophthal 113: 671-675. Brown DM, Nichols BE, Weingeist TA, Sheffield VC, Kimura AE & Stone EM (1992) Procollagen II gene mutation in Stickler syndrome. Arch Ophthalmol 110: 1589-1593. Brown DM, Vandenburgh K, Kimura AE, Weingeist TA, Sheffield VC & Stone EM (1995a) Novel frameshift mutations in the procollagen 2 gene (COL2A1) associated with Stickler syndrome (hereditary arthro-ophthalmopathy). Hum Mol Genet 4: 141-142. 61 Brown KS, Cranley RE, Greene R, Kleinman HK & Pennypacker JP (1981) Disproportionate micromelia (Dmm): an incomplete dominant mouse dwarfism with abnormal cartilage matrix. J Embryol Exp Morphol 62: 165-182. Bruckner P, Mendler M, Steinmann B, Huber S & Winterhalter KH (1988) The structure of human collagen type IX and its organization in fetal and infant cartilage fibrils. J Biol Chem 263: 16911-16917. Bruckner P, Vaughan L & Winterhalter KH (1985) Type IX collagen from sternal cartilage of chicken embryo contains covalently bound glycosaminoglycans. Proc Natl Acad Sci, USA 82: 2608-2612. Brunner HG, van Beersum SE, Warman ML, Olsen BR, Ropers HH & Mariman EC (1994) A Stickler syndrome gene is linked to chromosome 6 near the COL11A2 gene. Hum Mol Genet 3: 1561-1564. Buckwalter JA (1995) Aging and degeneration of the human inervertebral disc. Spine 20: 13071314. Bulleid NJ, Wilson R & Lees JF (1996) Type-III procollagen assembly in semi-intact cells: chain association, nucleation and triple-helix folding do not require formation of inter-chain disulphide bonds but triple-helix nucleation does require hydroxylation. Biochem J. 317: 195202. Bulleid NJ (1996) Novel assembly to study the initial events in the folding and assembly of procollagen. Seminars in Cell & Developmental Biology 7: 667-672. Burgeson RE, Lunstrum GP, Rokosova B, Rimberg CS, Rosenbaum LM & Keene DR (1990) The structure and function of type VII collagen. In: Fleischmajer R, Olsen BR & Kühn K (eds) Annals of the New York Academy of Sciences, vol. 580. Structure, molecular biology and pathology of collagen. The New York Academy of Sciences, New York p. 32-43. Chemke J, Carmi R, Galil A, Bar-Ziv Y, Ben-Ytzhak I & Zurkowski L (1992) WeissenbacherZweymüller syndrome: a distinct autosomal recessive skeletal dysplasia. Am J Med Genet 43: 989-995. Chen H, Yang SS & Gonzalez E (1980) Knist dysplasia: neonatal death with decropsy. Am J Med Genet 6: 171-178. Chu M-L, Pan T-C, Conway D, Saitta B, Stokes D, Kuo H-J, Glanville RW, Timpl R, Mann K & Deutzmann R (1990) The structure of type VI collagen. In: Fleischmajer R, Olsen BR & Kühn K (eds) Annals of the New York Academy of Sciences, vol. 580. Structure, molecular biology and pathology of collagen. The New York Academy of Sciences, New York p. 55-63. Chu M-L & Prockop DJ (1993) Collagen: gene structure. In: Royce PM & Steinmann B (eds) Connective tissue and its heritable disorders. Molecular, genetic and medical aspects. WileyLiss, New York p. 149-165. Clerget-Darpoux F, Bonaiti-Pellie C & Hochez J (1986) Effects of misspecifying genetic parameters in lod score analysis. Biometrics 42: 393-399. Constantinou CD, Pack M, Young SB & Prockop DJ (1990) Phenotypic heterogeneity in osteogenesis imperfecta: the mildly affected mother of a proband with a lethal variant has the same mutation subtituting cysteine for α1-glycine904 in a type I procollagen gene (COL1A1). Am J Hum Genet 47: 670-679. Cortina H, Aparici R, Beltran J & Alberto C (1977) The Weissenbacher-Zweymüller syndrome. A case report with review of the world literature. Pediatr Radiol 6: 109-111. Cotton RGH (1989) Detection of single base changes in nucleic acids. Biochem J 263: 1-10. Cotton RGH (1993) Current methods of mutation detection. Mutat Res 285: 125-144. Cotton RGH, Rodrigues NR & Campbell RD (1988) Reactivity of cytosine and thymine in singlebase-pair mismatches with hydroxylamine and osmium tetroxide and its application to the study of mutations. Proc Natl Acad Sci USA 85: 4397-4401. Creamer P & Hochberg MC (1997) Osteoarthritis. Lancet 350: 503-509. Cremer MA, Rosloniec EF & Kang AH (1998) The cartilage collagens: a review of their structure, organization, and role in the pathogenesis of experimental arthritis in animals and in human rheumatic disease. J Mol Med 76: 275-288. Deere M, Blanton SH, Scott CI, Langer LO, Pauli RM & Hecht JT (1995) Genetic heterogeneity in multiple epiphyseal dysplasia. Am J Hum Genet 56: 698-704. 62 Diab M, Wu J-J & Eyre DR (1996) Collagen type IX from human cartilage: a structural profile of intermolecular cross-linking sites. Biochem J 314: 327-332. Ellis LA, Taylor GR, Banks R & Baumberg S (1994) MutS binding protects heteroduplex DNA from exonuclease digestion in vitro: a simple method for detection of mutations. Nucleic Acid Res 22: 2710-2711. Eng C & Vijg J (1997) Genetic testing: the problems and the promises. Nat Biotechnol 15: 422426. Eyre DR (1991) The collagens of articular cartilage. Semin Arthritis Rheum 21: 2-11. Eyre DR, Apon S, Wu J-J, Ericsson LH & Walsh KA (1987) Collagen type IX: ecidence for covalent linkages to type II collagen in cartilage. FEBS Lett 220: 337-341. Eyre DR & Muir H (1977) Quantitative analysis of types I and II collagens in human intervertebral discs at various ages. Biochim Biophys Acta 492: 29-42. Eyre DR, Upton MP, Shapiro FD, Wilkinson RH & Vawter GF (1986) Nonexpression of cartilage type II in a case of Langer-Saldino achondrogenesis. Am J Hum Genet 39: 52-67. Eyre DR & Wu J-J (1987) Type XI or 1α2α3α collagen. In: Mayne R & Burgeson RE (eds) Structure and function of collagen types. Academic Press, Inc. p. 261-281. Eyre DR & Wu J-J (1995) Collagen structure and cartilage matrix integrity. J Rheumatol 22: 82-88. Fässler RP, Schnegelsberg NJ, Dausman J, Shinya T, Muragaki Y, McCarthy MT, Olsen BR & Jaenisch R (1994) Mice lacking α1(IX) collagen develop noninflammatory degenerative joint disease. Proc Natl Acad Sci, USA 91:5070-5074. Fernandez RJ, Wilkin DJ, Weis MA, Wilcox WR, Cohn DH, Rimoin DL & Eyre DR (1998) Incorporation of structurally defective type II collagen into cartilage matrix in Kniest chondrodysplasia. Arch Biochem Biophys 355: 282-290. Fichard A, Kleman J-P & Ruggiero F (1994) Another look at collagen V and XI molecules. Matrix Biol 14: 515-531. Fischer SG & Lerman LS (1983) DNA fragments differing by single base-pair substitutions are separated in denaturing gradient gels: correspondence with melting theory. Proc Natl Acad Sci USA 80: 1579-1583. Francomano CA, Liberfarb RM, Hirose T, Maumenee IH, Streeten EA, Meyers DA & Pyeritz RE (1987) The Stickler syndrome: evidence for close linkage to the structural gene for type II collagen. Genomics 1: 293-296. Ganguly A & Prockop DJ (1990) Detection of single-base mutations by reaction of DNA heteroduplexes with water-soluble carbodiimide followed by primer extension: application to products from the polymerase chain reaction. Nucleic Acid Res 18: 3933-3939. Ganguly A & Prockop DJ (1995) Detection of mismatched bases in double stranded DNA by gel electrophoresis. Electrophoresis 16: 1830-1835. Ganguly A, Rock MJ & Prockop DJ (1993) Conformation-sensitive gel electrophoresis for rapid detection of single-base differences in double-stranded PCR products and DNA fragments: evidence for solvent-induced bends in DNA heteroduplexes. Proc Natl Acad Sci USA 90: 10325-10329. Ganguly A, Rooney JE, Hosomi S, Zeiger AR & Prockop DJ (1989) Detection and location of single-base mutations in large DNA fragments by immunomicroscopy. Genomics 4: 530-538. Garofalo S, Metsäranta M, Ellard J, Smith C, Horton W, Vuorio E & de Crombrugghe B (1993) Assembly of cartilage collagen fibrils is disrupted by overexpression of normal type II collagen in transgenic mice. Proc Natl Acad Sci USA 90: 3825-3829. Garofalo S, Vuorio E, Metsäranta M, Rosati R, Toman D, Vaughan J, Lozano G, Mayne R, Ellard J, Horton W & de Crombrugghe B (1991) Reduced amounts of cartilage collagen fibrils and growth plate anomalies in transgenic mice harboring a glycine-to-cysteine mutation in the mouse type II procollagen α1-chain gene. Proc Natl Acad Sci USA 88: 9648-9652. Geschwind DH, Rhee R & Nelson SF (1996) A biotinylated MutS fusion protein and its use in a rapid mutation screening technique. Genet Anal 13: 105-111. Giedion A, Brandner M, Lecannellier J, Muhar U, Prader A, Sulzer J & Zweymüller E (1982) Otospondylo-megaepiphyseal dysplasia (OSMED). Hlev Paediat Acta 37: 361-380. 63 Gilbert-Barnes E, Langer LO Jr, Opitz JM, Laxova R & Sotelo-Arila C (1996) Kniest dysplasia: radiologic, histopathological, and scanning electronmicroscopic findings. Ann J Med Genet 63: 34-45. Glavac D & Dean M (1995) Applications of heteroduplex analysis for mutation detection in disease genes. Hum Mutat 6: 281-287. Godfrey M & Hollister TW (1988) Type II achondrogenesis-hypochondrogenesis: identification of abnormal type II collagen. Am J Hum Genet 43: 904-913. Godfrey M, Keene DR, Blank E, Hori H, Sakai LY, Sherwin LA & Hollister DW (1988) Type II achondrogenesis-hypochondrogenesis: morphologic and immunohistopathologic studies. Am J Hum Genet 43: 894-903. Gotoh M, Hasebe M, Ohira T, Hasegawa Y, Shinohara Y, Sota H, Nakao J & Tosu M (1997) Rapid method for detection of point mutations using mismatch binding protein (MutS) and an optical biosensor. Genet Anal 14: 47-50. Griffith AJ, Sprunger LK, Sirko-Osadsa DA, Tiller GE, Meisler MH & Warman ML (1998) Marshall syndrome associated with a splicing defect at the COL11A1 locus. Am J Hum Genet 62: 816-823. Grover J, Chen XN, Korenberg JR & Roughley PJ (1995) The human lumican gene. Organization, chromosomal location, and expression in articular cartilage. J Biol Chem 270: 21942-21949. Grundmann K, Zimmermann B, Barrach HJ & Merker HJ (1980) Behaviour of epiphyseal mouse chondrocyte populations in monolayer culture. Morphological and immunohistochimical studies. Virchows Arch 389: 167-187. Hacia JG (1999) Resequencing and mutational analysis using oligonucleotide microarrays. Nat Genet 21 Suppl 1: 42-47. Haga N, Nakamura K, Takikawa K, Manabe N, Ikegawa S & Kimizuka M (1998) Stature and severity in multiple epiphyseal dysplasia. J Pediatr Orthop 18: 394-397. Hagg R, Hedbom E, Möllers U, Aszódi A, Fässler R & Bruckner P (1998) Absence of the α1(IX) chain leads to a functional knock-out of the entire collagen IX protein in mice. J Biol Chem 272: 20650-20654. Haimes HB, Jimenez PA, Shinya T & Olsen BR (1995) Overexpression of the NC4 domain of type IX collagen induces osteoarthitis in mice. Inflamm Res 44 Suppl 2: S127-128. Hanke M & Wink M (1994) Direct DNA sequencing of PCR-amplified vector inserts following enzymatic degradation of primers and dNTPs. Biotechniques 17: 858-860. Hanson IM, Gorman P, Lui VC, Cheah KS, Solomon E & Trowsdale J (1989) The human alpha 2(XI) collagen gene (COL11A2) maps to the centromeric border of the major histocompatibility complex on chromosome 6. J Biol Chem 264: 13910-13916. Hardingham TE & Fosang AJ (1992) Proteoglycans: many forms and many functions. FASEB J 6: 861-870. Hardingham TE & Fosang AJ (1995) The structure of aggrecan and its turnover in cartilage. J Rheumatol Suppl 43: 86-90. Harrod MJ, Friedman JM, Currarino G, Pauli RM & Langer JO Jr (1984) Genetic heterogeneity in spondyloepiphyseal dysplasia congenita. Am J Med Genet 18: 311-320. Hasue M (1993) Pain and the nerve root. An interdisciplinary approach. Spine 18: 2053-2058. Hayward-Lester A, Oefner PJ, Sabatini S & Doris PA (1995) Accurate and absolute quantitative measurement of gene expression by single-tube RT-PCR and HPLC. Genome Res 5: 494-499. Hecht JT, Francomano CA, Briggs MD, Deere M, Conner B, Horton WA, Warman M, Cohn DH & Blanton SH (1993) Linkage of typical pseudoachondroplasia to chromosome 19. Genomics 18: 661-666. Hecht JT, Nelson LD, Crowder E, Wang Y, Elder FFB, Harrison WR, Francomano CA, Prange CK, Lennon GG, Deere M & Lawler J (1995) Mutations in exon 17B of cartilage oligomeric matrix protein (COMP) cause pseudoachondroplasia. Nat Genet 10: 325-329. Heinegård D & Oldberg Å (1989) Structure and biology of cartilage and bone matrix noncollagenous macromolecules. FASEB J 3: 2042-2051. Heliövaara M (1989) Risk factors for low back pain and sciatica. Ann Med 21: 257-264. Heliövaara M, Impivaara O, Sievers K, Melkas T, Knekt P, Korpi J & Aromaa A (1987) Lumbar disc syndrome in Finland. J Epidemiol community Health 41: 251-258. 64 Henry I, Bernheim A, Bernard M, van der Rest M, Kimura T, Jeanpierre C, Barichard F, Berger R, Olsen BR, Ramirez F & Junien C (1988) Mapping of a human fibrillar collagen gene, pro α1(XI) (COL11A1), to the p21 region of chromosome 1. Genomics 3: 87-90. Herrmann J, France TD, Spranger JW, Opitz JM & Wiffler C (1975) The Stickler syndrome (Hereditary arthroophthalmopathy). Birth Defects 11: 76-103. Hoefnagel D, Sycamore LK, Russell SW & Bucknall WE (1967) Hereditary multiple epiphyseal dysplasia. Ann Hum Genet 30: 201-210. Horton WA & Hecht JT (1993) The chondrodysplasias. In: Royce PM & Steinmann B (eds) Connective tissue and its heritable disorders. Molecular, genetic and medical aspects. WileyLiss, New York p 641-675. Horton WA & Rimoin DL (1979) Kniest dysplasia. A histochemical study of the growth plate. Pediatr Res 13: 1266-1270.s Huber S, van der Rest M, Bruckner P, Rodriguez E, Winterhalter KH & Vaughan L (1986) Identification of the type IX collagen polypeptide chains. The alpha 2(IX) polypeptide carries the chondroitin sulfate chain(s). J Biol Chem 261: 5965-5968. Humzah MD & Soames RW (1988) Human intervertebral disc: structure and function. Anat Rec 220: 337-356. Ikegawa S, Ohashi H, Nishimura G, Kim KC, Sannohe A, Kimizuka M, Fukushima Y, Nagai T & Nakamura Y (1998) Novel and recurrent COMP (cartilage oligomeric matrx protein) mutations in pseudoachondroplasia and multiple epiphyseal dysplasia. Hum Genet 103: 633-638. International Working Group on Constitutional Diseases of Bone (1998) International nomenclature and classification of the osteochondrodysplasias (1997). Am J Med Genet 79: 376-382. Jensen MC, Brant-Zawadzki MN, Obuchowski N, Modic MT, Malkasian D & Ross JS (1994) Magnetic resonance imaging of the lumbar spine in people without back pain. N Engl J Med 331: 69-73. Kääriäinen H, Barrow M & Hennekam R (1993) Bone dysplasia, midface hypoplasia, and deafness: three new patients and review of the literature. Am J Med Genet 46: 223-227. Kainulainen K, Perola M, Terwilliger J, Kaprio J, Koskenvuo M, Syvänen AC, Vartiainen E, Peltonen L & Kontula K (1999) Evidence for involvement of type 1 angiotensin II receptor licus in essential hypertension, Hypertension 33: 844-849. Keene DR, Oxford JT & Morris NP (1995) Ultrastructural localization of collagen types II, IX, and XI in the growth plate of human rib and fetal bovine epiphyseal cartilage: type XI is restricted to thin fibrils. J Histochem Cytochem 43: 967-979. Kellgren JH, Lawrence JS & Bier F (1963) Genetic factors in generalized osteo-arthrosis. Ann Rheum Dis 22: 237-255. Kielty CM, Hopkinson I & Grant ME (1993) Collagen: the collagen family: structure, assembly, and organixation in extracellular matrix. In: Royce PM & Steinmann B (eds) Connective tissue and its heritable disorders. Molecular, genetic and medical aspects. Wiley-Liss, New York, p 103-147. Kimata K, Barrach HJ, Brown KS & Pannypacker JP (1981) Absence of proteoglycan core protein in cartilage from the cmd/cmd (cartilage matrix deficiency) mouse. J Biol Chem 256: 69616968. Kimura T, Cheah KS, Chan SD, Lui VC, Mattei MG, van der Rest M, Ono K, Solomon E, Ninomiya Y & Olsen BR (1989) The human alpha 2(XI) collagen (COL11A2) chain. Molecular cloning of cDNA and genomic DNA reveals characteristics of a fibrillar collagen with differences in genomic organization. Genomics 5: 925-931. Kimura T, Nakata K, Tsumaki N, Miyamoto S, Matsui Y, Ebara S & Ochi T (1996) Progressive degeneration of articular cartilage and intervertebral discs. An experimental study in transgenic mice bearing a type IX collagen mutation. Int Orthop 20: 177-181. Kinsella MG, Tsoi CK, Järveläinen HT & Wight TN (1997) Selective expression and processing of biglycan during migration of bovine aortic endothelial cells. The role of endogenous basic fibroblast growth factor. J Biol Chem 272: 318-325. 65 Kivirikko KI (1995) Posttranslational processing of collagens. In: Bittar EE & Bittar N (eds) Principles of medical biology, vol. 3. Cellular organelles and the extracellular matrix. JAI Press, London p 233-254. Kivirikko S, Saarela J, Myers JC, Autio-Harmainen H & Pihlajaniemi T (1995) Distribution of type XV collagen transcripts in human tissue and their production by muscle cells and fibroblasts. Am J Pathol 147: 1500-1509. Knowlton RG, Katzenstein PL, Moskowitz RW, Weaver EJ, Malemud CJ, Pathria MN, Jimenez SA & Prockop DJ (1990) Genetic linkage of a polymorphsm in the type II procollagen gene (COL2A1) to primary osteoarthritis associated with mild chondrodysplasia. N Engl J Med 322: 526-530. Knowlton RG, Weaver EJ, Struyk AF, Knobloch WH, King RA, Norris K, Shamban A, Uitto J, Jimenez SA & Prockop DJ (1989) Genetic linkage analysis of hereditary arthro-ophthalmopathy (Stickler syndrome) and the type II procollagen gene. Am J Hum Genet 45: 681-688. Körkkö J, Ala-Kokko L. DePaepe A, Nyutick L, Earley J & Prockop DJ (1998) Analysis of the COL1A1 and COL1A2 genes by PCR amplification and scanning by conformation-sensitive gel electrophoresis identifies only COL1A1 mutations in 15 patients with osteogenesis imperfecta type I: identification of common sequences of null-allele mutations. Am J Hum Genet 62: 98110. Körkkö J, Cohn DH, Ala-Kokko L, Krakow D & Prockop DJ Widely distributed mutations in the COL2A1 gene produce achondrogenesis type II/hypochondrogenesis. Submitted. Körkkö J, Kuivaniemi H, Paassilta P, Zhuang J, Tromp G, DePaepe A, Prockop DJ & Ala-Kokko L (1997) Two recurrent nucleotide mutations in the COL1A1 gene is four patients with osteogenesis imperfecta: about one-fifth are recurrent. Hum Mutat 9: 148-156. Körkkö J, Ritvaniemi P, Haataja L, Kääriäinen H, Kivirikko KI, Prockop DJ & Ala-Kokko L (1993) Mutation in type II procollagen (COL2A1) that substitutes aspartate for glycine α1-67 and that causes cataracts and retinal detachment: evidence for molecular heterogeneity in the Wagner syndrome and the Stickler syndrome (arthro-ophthalmopathy). Am J Hum Genet 53: 55-61. Kuivaniemi H, Tromp G & Prockop DJ (1997) Mutations in fibrillar collagens (types I, II, III, and XI), fibril-associated collagen (type IX), and network-forming collagen (type X) cause a spectrum of diseases of bone, cartilage, and blood vessels. Hum Mutat 9: 300-315. Langer LO Jr, Spranger JW, Greinacher I & Herdman RC (1969) Thanatophoric dwarfism. A condition confused with achondroplasia in the neonate, with brief comments on achondrogenesis and homozygous achondroplasia. Radiology 92: 285-294. Lee B, Vissing H, Ramirez F, Rogers D & Rimoin D (1989) Identification of the molecular defect in a family with spondyloepiphyseal dysplasia. Science 244: 978-980. Lees JF, Tasab J & Bulleid NJ (1997) Identification of the molecular recognition sequence which determines the type-specific assembly of procollagen. EMBO J. 16: 908-916. Li S-W, Prockop DJ, Helminen H, Fässler R, Lapveteläinen T, Kiraly K, Peltarri A, Arokoski J, Lui H, Arita M & Khillan JS (1995) Transgenic mice with targeted inactivation of the Col2a1 gene for collagen II develop a skeleton with membranous and periosteal bone but no endochondral bone. Genes Dev 9: 2821-2830. Li Y, Lacerda DA, Warman ML, Beier DR, Yoshioka H, Ninomiya Y, Oxford JT, Morris NP, Andrikopoulos K, Ramirez F, Wardell BB, Lifferth GD, Teuscher C, Woodward SR, Taylor BA, Seegmiller RE & Olsen BR (1995) A fibrillar collagen gene, Col11a1, is essential for skeletal morphogenesis. Cell 80: 423-430. Liberfarb RM & Goldblatt A (1986) Prevalence of mitral-valve prolapse in the Stickler syndrome. Am J Med Genet 24: 387-392. Liberfarb RM, Hirose T & Holmes LB (1979) The Wagner-Stickler syndrome - a genetic study. Birth Defects 15: 145-154. Lishanski A, Ostrander EA & Rine J (1994) Mutation detection by mismatch binding protein, MutS, in amplified DNA:application to the cystic fibrosis gene. Proc Natl Acad Sci USA 91: 2674-2678. 66 Liu W-O, Oefner PJ, Qian C, Odom RS & Francke U (1997/98) Denaturing HPLC-identified novel FBN1 mutations, polymorphisms, and sequence variants in Marfan syndrome and related connective tissue disorders. Genetic Testing 1: 237-242. Loughlin J, Irven C, Mustafa Z, Briggs MD, Carr A, Lynch SA, Knowlton RG, Cohn DH & Sykes B (1998) Identification of five novel mutations in cartilage oligomeric matrix protein gene in pseudoachondroplasia and multiple epiphyseal dysplasia. Hum Mutat Suppl 1: S10-S17. Lui VCH, Kong RYC, Nicholls J, Cheung ANY & Cheah KSE (1995) The mRNAs for the three chains of human collagen type XI are widely distributed but not necessarily co-expressed: implications for homotrimeric, heterotrimeric and heterotypic molecules. Biochem J 311: 511516. Lui VCH, Ng LJ, Sat EWY, Nicholls J & Cheah KSE (1996) Extensive alternative splicing within the amino-propeptide coding domain of α2(XI) procollagen mRNAs. J Biol Chem 271: 1694516951. Lyamichev V, Brow MA & Dahlberg JE (1993) Structure-specific endonucleotic cleavage of nucleic acids by eubacterial DNA polymerases. Science 260: 778-783. Maddox BK, Garofalo S, Smith C, Keene DR & Horton WA (1997a) Skeletal development in transgenic mice expressing a mutation at Gly574Ser of type II collagen. Dev Dyn 208: 170-177. Maddox BK, Keene DR, Sakai LY, Charbonneau NL, Morris NP, Ridgway CC, Boswell BA, Sussman MD, Horton WA, Bächinger HP & Hecht JT (1997b) The fate of cartilage oligomeric matrix protein is determined by the cell type in the case of a novel mutation in pseudoachondroplasia. J Biol Chem 272: 30993-30997. Maroteaux P, Stanescu V & Stanescu R (1983) Hypochondrogenesis. Eur J Pediatr 141: 14-22. Marshall A & Hodgson J (1998) DNA chips: an array of possibilities. Nat Biotechnol 16: 27-31. Marshall D (1958) Ectodermal dysplasia. Report of kindred with ocular abnormalities and hearing defect. Am J Ophthal 45: 143-156. Mashal RD, Koontz J & Sklar J (1995) Detection of mutations by cleavage of DNA heteroduplexes with bacteriophage resolvases. Nat Genet 9: 177-183. Mason RM & Palfrey AJ (1984) Intervetebral disc degeneration in adult mice with hereditary kyphoscoliosis J Orthop Res 2: 333-338. Mayne R (1989) Cartilage collagens. Arthritis Rheum 32: 241-246. Mayne R & Brewton RG (1993) New members of the collagen superfamily. Curr Opin Cell Biol 5: 883-890. Mayne R, Brewton RG, Mayne PM & Baker JR (1993) Isolation and characterization of the chains of type V/type XI collagen present in bovine vitreous. J Biol Chem 268: 9381-9386. McCormick D, van der Rest M, Goodship J, Lozano G, Ninomiya Y & Olsen BR (1987) Structure of the glycosaminoglycan domain in the type IX collagen-proteoglycan. Proc Natl Acad Sci, USA 84: 4044-4048. Mendler M, Eich-Bender SG, Vaughan L, Winterhalter KH & Bruckner P (1989) Cartilage contains mixed fibrils of collagen types II, IX and XI. J Cell Biol 108: 191-197. Metsäranta M, Garofalo S, Decker G, Rintala M, de Crombrugghe B & Vuorio E (1992) Chondrodysplasia in transgenic mice harboring a 15-amino acid deletion in the triple helical domain in proα1(II) collagen chain. J Cell Biol 118: 203-212. Moore KL (1992a) Clinically oriented anatomy, 3rd ed. Williams & Wilkins, Baltimore, p 774-778. Moore KL (1992b) Clinically oriented anatomy, 3rd ed. Williams & Wilkins, Baltimore, p 323351. Morris NP & Bächinger HP (1987) Type XI collagen is a heterotrimer with the composition (1α2α3α) retaining non-triple-helical domains. J Biol Chem 262: 11345-11350. Moskowitz RW (1989) Clinical and laboratory findings in osteoarthritis. In: McCarthy (ed) Arthritis and allied conditions, 11th ed. Lea & Febiger, Philadephia, p 1605-1630. van Mourik JBA, Buma P & Wilcox WR (1998b) Electron microscopical study in multiple epiphyseal dysplasia type II. Ultrastruct Pathol 22: 249-251. van Mourik JBA, Hamel BCJ & Mariman ECM (1998a) A large family with epiphyseal dysplasia linked to COL9A2 gene. Am J Med Genet 77: 234-240. Muir H (1995) The chondrocyte, architect of cartilage. Biomechanics, structure, function and molecular biology of cartilage matrix macromolecules. Bioessays 17: 1039-1048. 67 Mundlos S & Olsen BR (1997a) Heritable diseases of the skeleton. Part I: Molecular insights into skeletal development - transcription factors and signaling pathways. FASEB J 11: 125-132. Mundlos S & Olsen BR (1997b) Heritable diseases of the skeleton. Part II: Molecular insights into skeletal development - matrix components and their homeostasis. FASEB J 11: 227-233. Muragaki Y, Kimura T, Ninomiya Y & Olsen BR (1990) The complete primary structure of two distinct forms of human α1(IX) collagen chains. Eur J Biochem 192: 703-708. Muragaki Y, Mariman ECM, van Beersum SEC, Perälä M, van Mourik JBA, Warman ML, Olsen BR & Hamel BCJ (1996) A mutation in the gene encoding the α2 chain of the fibril-associated collagen IX, COL9A2, causes multiple epiphyseal dysplasia (EDM2). Nat Genet 12: 103-105. Murray LW; Bautista J, James PL & Rimoin DL (1989) Type II collagen defects in the chondrodysplasias. I. Spondyloepiphyseal dysplasias. Am J Hum Genet 45: 5-15. Myers RM, Maniatis T & Lerman SL (1987) Detection and localization of single base changes by denaturing gradient gel electrophoresis. In: Wu R (ed) Methods in Enzymology, Vol. 155. Academic Press, San Diego, p 501-527. Nah HD & Upholt WB (1991) Type II collagen mRNA containing an alternatively spliced exon predominates in the chick limb prior to chondrogenesis. J Biol Chem 266: 23446-23452. Nakata K, Ono K, Miyazaki J-I, Olsen BR, Muragaki Y, Adachi E, Yamamura K-I & Kimura T (1993) Osteoarthritis associated with mild chondrodysplasia in transgenic mice expressing α1(IX) collagen chains with a central deletion. Proc Natl Acad Sci USA 90: 2870-2874. Neame PJ & Barry FP (1993) The link proteins. Experientia 49: 393-402. Neame PJ, Young CN & Treep JT (1990) Isolation and primary structure of PARP, a 24-kDa proline and arginine-rich protein from bovine cartilage closely related to the NH2-terminal domain in collagen α1(XI). J Biol Chem 265: 20401-20408. Nerlich AG, Boos N, Wiest I & Aebi M (1998) Immunolocalization of major interstitial collagen types in human intervertebral discs of various ages. Virchows Arch 432: 67-76. Newall JF & Ayad S (1995) Collagen IX isoforms in the intervertebral disc. Biochem Soc Trans 23: 517S. Newton G, Weremowicz S, Morton CC, Copeland NG, Gilbert DJ, Jenkins NA & Lawler J (1994) Characterization of human and mouse cartilage oligomeric matrix protein. Genomics 24: 435439. Nishimura I, Muragaki Y & Olsen BR (1989) Tissue-specific forms of type IX collagenproteoglycan arise from the use of two widely separated promoters. J Biol Chem 264: 2003320041. Niyibizi C & Eyre DR (1989) Identification of the cartilage α1(XI) chain in the type V collagen from bovine bone. FEBS Lett 242: 314-318. Nollau P & Wagener C (1997) Methods for detection of point mutations: performance and quality assessment. IFCC Scientific Division, Committee on Molecular Biology Techniques. Clin Chem 43: 1114-1128. Novack DF, Casna NJ, Fischer SG & Ford JP (1986) Detection of single base-pair mismatches in DNA by chemical modification followed by electrophoresis in 15% polyacrylamide gel. Proc Natl Acad Sci USA 83: 586-590. O’Donnell JJ, Sirkin S & Hall BD (1976) Generalized osseous abnormalities in the Marshall syndrome. Birth Defects 12: 299-314. O’Donovan MC, Oefner PJ, Roberts SC, Austin J, Hoogendoorn B, Guy C, Speight G, Upadhyaya M, Sommer SS & McGuffin P (1998) Blind analysis of denaturing high-performance liquid chromatography as a tool for mutation detection. Genomics 52: 44-49. Oehlmann R, Summerville GP, Yeh G, Weaver EJ, Jimenez SA & Knowlton RG (1994) Genetic linkage mapping of multiple epiphyseal dysplasia to the pericentromeric region of chromosome 19. Am J Hum Genet 54: 3-10. O’Reilly MS, Boehm T, Shing Y, Fukai N, Vasios G, Lane WS, Flynn E, Birkhead JR, Olsen BR & Folkman J (1997) Endostatin: an endogenous inhibitor of angiogenesis and tumour growth. Cell 88: 277-285. Orita M, Iwahana H, Kanazawa H, Hayashi K & Sekiya T (1989a) Detection of polymorphisms of human DNA by gel electrophoresis as single-stranded conformation polymorphisms. Proc Natl Acad Sci USA 86: 2766-2770. 68 Orita M, Suzuki Y, Sekiya T & Hayashi K (1989b) Rapid and sensitive detection of point mutations and DNA polymorphisms using the polymerase chain reaction. Genomics 5: 874-879. Paassilta P, Lohiniva J, Annunen S, Bonaventure S, Le Merrer M, Pai L & Ala-Kokko L (1999a) COL9A3: a third locus for multiple epiphyseal dysplasia. Am J Hum Genet 64: 1036-1044. Paassilta P, Pihlajamaa T, Annunen S, Brewton RG, Wood BM, Johnson CC, Liu J, Gong Y, Warman ML, Prockop DJ, Mayne R & Ala-Kokko L (1999b) Complete sequence of 23 kb human COL9A3 gene. Detection of Gly-X-Y triplet deletions which represent neutral variants. J Biol Chem, in press. Pace JM, Li Y, Seegmiller RE, Teuscher C, Taylor BA & Olsen BR (1997) Disproportionate micromelia (Dmm) in mice caused by a mutation in the C-propeptide coding region of Col2a1. Dev Dyn 208: 25-33. Palotie A, Väisänen P, Ott J, Ryhänen L, Elima K, Vikkula M, Cheah K, Vuorio E & Peltonen L (1989) Predisposition to familial osteoarthrosis linked to type II collagen gene. Lancet 1: 924927. Perälä M, Elima K, Metsäranta M, Rosati R, de Crombrugghe B & Vuorio E (1994) The exon structure of the mouse α2(IX) gene shows unexpected divergence from the chick gene. J Biol Chem 269: 5064-5071. Perälä M, Hänninen M, Hästbacka J, Elima K & Vuorio E (1993) Molecular cloning of the human α2(IX) collagen cDNA and assignment of the human COL9A2 gene to chromosome 1. FEBS Lett 319: 177-180. Pihlajamaa T, Prockop DJ, Faber J, Winterpacht A, Zabel B, Giedion A, Wiesbauer P, Spranger J & Ala-Kokko L (1998b) Heterozygous glycine substitution in the COL11A2 gene in the original patient with the Weissenbacher-Zweymüller syndrome demonstrates its identity with heterozygous OSMED (nonocular Stickler syndrome). Am J Med Genet 80: 115-120. Pihlajamaa T, Vuoristo MM, Annunen S, Perälä M, Prockop DJ & Ala-Kokko L (1998a) Human COL9A1 and COL9A2 genes. Two genes of 90 and 15 kb code for similar polypeptides of the same collagen molecule. Matrix Biol 17:237-241. Pihlajaniemi T & Rehn M (1995) Two new collagen subgroups: membrane-associated collagens and types XV and XVIII. Prog Nucleic Acid Res Mol Biol 50: 225-262. Poole AR, Pidoux I, Reiner A, Rosenberg L, Hollister D, Murray L & Rimoin D (1988) Kniest dysplasia is characterized by an apparent abnormal processing of the C-propeptide of type II cartilage collagen resulting in imperfect fibril assembly. J Clin Invest 81: 579-589. Prockop DJ & Kivirikko KI (1995) Collagens: molecular biology, diseases, and potentials for therapy. Annu Rev Biochem 64: 403-434. Ramsay G (1998) DNA chips: state-of-the art. Nat Biotechnol 16: 40-44. Ren ZX, Brewton RG & Mayne R (1991) An analysis by rotary shadowing of the structure of the mammalian vitreous humor and zonular apparatus. J Struct Biol 106: 57-63. Richards AJ, Yates JRW, Williams R, Payne SJ, Pope FM, ScottJd & Snead MP (1996) A family with Stickler syndrome type 2 has a mutation in the COL11A1 gene resulting in the substitution of glycine 97 by valine in α1(XI) collagen. Hum Mol Genet 5: 1339-1343. Risch N & Giuffra L (1992) Model misspecification and multipoint linkage analysis. Hum Hered 42: 77-92. Rittenhouse E, Dunn LC, Cookingham J, Calo C, Spiegelman M, Dooher GB & Bennett D (1978) Cartilage matrix deficiency (cmd): a new autosomal recessive lethal mutation in the mouse. J Embryol Exp Morphol 43: 71-84. Ritvaniemi P, Hyland J, Ignatius J, Kivirikko KI, Prockop DJ & Ala-Kokko L (1993) A fourth example suggests that premature termination codons in the COL2A1 gene are a common cause of the Stickler syndrome. Analysis of the COL2A1 gene by denaturing gradient gel electrophoresis. Genomics 17: 218-221. Ritvaniemi P, Körkkö J, Bonaventure J, Vikkula M, Hyland J, Paassilta P, Kaitila I, Kääriäinen H, Sokolov BP, Hakala M, Mannismäki P, Meerson EM, Klemola T, Williams C, Peltonen L, Kivirikko KI, Prockop DJ & Ala-Kokko L (1995) Identification of COL2A1 gene mutations in patients with chondrodysplasias and familial osteoarthritis. Arthritis Rheum 38: 999-1004. Roberts S, Menage J, Duance V, Wotton S & Ayad S (1991) Collagen types around the cells of the intervertebral disc and cartilage end plate: an immunolocalization study. Spine 16: 1030-1038. 69 Roest PA, Roberts RG, Sugino S, van Ommen GJ & den Dunnen JT (1993) Protein truncation test (PTT) for rapid detection of translation-terminating mutations. Hum Mol Genet 2: 1719-1721. Rokos I, Muragaki Y, Warman ML & Olsen BR (1994) Assembly and sequencing of a cDNA covering the entire mouse α1(IX) collagen chain. Matrix Biol 14: 1-8. Roughley PJ & Lee ER (1994) Cartilage proteoglycans: structure and potential functions. Microsc Res Tech 28: 385-397. Ryan MC & Sandell LJ (1990) Differential expression of a cysteine-rich domain in the aminoterminal propeptide of type II (cartilage) procollagen by alternative splicing of mRNA. J Biol Chem 265: 10334-10339. Saarela J, Rehn M, Oikarinen A, Autio-Harmainen H & Pihlajaniemi T (1998) The short and long forms of type XVIII collagen show clear tissue specificities in their expression and location in basement membrane zones in humans. Am J Pathol 153: 611-626. Saldino RM (1971) Lethal short-limbed dwarfism: achondrogenesis and thanatophoric dwarfism. Am J Roentgenol Radium Ther Nucl Med 112: 185-197. Sambrook PN, MacGregor AJ & Spector TJ (1999) Genetic influences on cervical and lumbar disc degeneration: a magnetic resonance imaging study in twins. Arthritis Rheum 42: 366-372. Sandell LJ, Morris N, Robbins JR & Goldring MB (1991) Alternatively spliced type II procollagen mRNAs define distinct populations of cells during vertebral development: differential expression of the amino-propeptide. J Cell Biol 114: 1307-1319. Scapinelli R (1993) Lumbar disc herniation in eight siblings with a positive family history for disc disease. Acta Orthop Belg 59: 371-376. Schiller AL (1994) Bones and joints. In: Rubin E & Farber JL (eds) Pathology, 2nd ed. J.B. Lippincott, Philadelphia p 1273-1346. Seegmiller RE, Fraser FC & Sheldon H (1971) A new chondrodystrophic mutant in mice. J Cell Biol 48: 580-593. Seery CM & Davison PF (1991) Collagens of the bovine vitreous. Invest Ophthalmol Vis Sci 32: 1540-1550. Shanske AL, Bogdanow A, Shprintzen RJ & Marion RW (1997) The Marshall syndrome. Report of a new family and review of the literature. Am J Med Genet 70: 52-57. Shanske A, Bogdanov A, Shprintzen RJ & Marion RW (1998) Marshall syndrome and a defect at the COL11A1 locus (letter). Am J Hum Genet 63: 1558-1559. Shaw LM & Olsen BR (1991) FACIT collagens: diverse molecular bridges in extracellular matrices. Trends Biochem Sci 16: 191-194. Sheffield VC, Cox DR, Lerman LS & Myers RM (1989) Attachment of a 40-base-pair G+C-rich sequence (GC-clamp) to genomic DNA fragments by the polymerase chain reaction results in improved detection of single-base changes. Proc Natl Acad Sci USA 86: 232-236. Sirko-Osadsa DA, Murray MA, Scott JA, Lavery MA, Warman ML & Robin NH (1998) Stickler syndrome without eye involvement is caused by mutations in COL11A2, the gene encoding the α2(XI) chain of type XI collagen. J Pediatr 132: 368-371. Slepecky NB, Cefaratti LK & Yoo TJ (1992a) Type II and type IX collagen form heterotypic fibers in the tectorial membrane of the inner ear. Matrix 11: 80-86. Slepecky NB, Savage JE & Yoo TJ (1992b) Localization of type II, IX and V collagen in the inner ear. Acta Otolaryngol (Stockh) 112: 611-617. Snead MP, Payne SJ, Barton DE, Yates JRW, Al-Imara L, Pope FM & Scott JD (1994) Stickler syndrome: correlation between vitreoretinal phenotypes and linkage to COL2A1. Eye 8: 609614. Snead MP & Yates JRW (1999) Clinical and molecular genetics of Stickler syndrome. Am J Med Genet 36: 353-359. Spranger J (1998) The type XI collagenopathies. Pediatr Radiol 28: 745-750. Spranger JW, Langer LO & Wiedemann H-R (1974) Bone dysplasias. An atlas of constitutional disorders of skeletal development. WB Saunders Co., Philadelhia. Spranger J, Winterpacht A & Zabel B (1994) Type II collagenopathies: a spectrum of chondrodysplasias. Eur J Pediatr 153: 56-65. Spranger J, Winterpacht A & Zabel B (1997) Kniest dysplasia: Dr. W. Kniest, his patient, the molecular defect. Am J Med Genet 69: 79-84. 70 Stanescu R, Stanescu V, Muriel M-P & Maroteaux (1993) Multiple epiphyseal dysplasia, Fairbank type:morphologic and biochemical study of cartilage. Am J Med Genet 45: 501-507. Stanescu V (1990) The small proteoglycans of cartilage matrix. Semin Arthitis Rheum 20 (Suppl. 1): 51-64. Stanescu V, Maroteaux P & Stanescu R (1982) The biochemical defect of pseudoachondroplasia. Eur J Pediatr 138: 221-225. Stecher RM (1941) Heberden’s nodes. Heredity in hypertrophic arthritis of the finger joints. Am J Med Sci 201: 801-809. Stecher RM, Hersh AH & Hauser H (1953) Heberden’s nodes. The family history and radiographic appearance of a large family. Am J Hum Genet 5: 46-60. van Steensel MAM, Buma P, de Waal Malefijt MC, van den Hoogen FHJ & Brunner HG (1997) Oto-spondylo-megaepiphyseal dysplasia (OSMED): clinical description of three patients homozygous for a missense mutation in the COL11A2 gene. Am J Med Genet 70: 315-323. Stickler GB, Belau PG, Farrell FJ, Jones JD, Pugh DG, Steinberg AG & Ward LE (1965) Hereditary progressive arthro-ophthalmopathy. Mayo Clin Proc 40: 433-455. Stickler GB & Pugh DG (1967) Hereditary progressive arthro-ophthalmopathy II. Additional observations on vertebral abnormalities, a hearing defect, and a report of a similar case. Mayo Clin Proc 42: 495-500. Stratton RF, Lee B & Ramirez F (1991) Marshall syndrome. Am J Med Genet 41: 35-38. Swann DA & Sotman SS (1980) The chemical composition of bovine vitreous-humour collagen fibres. Biochem J 185: 545-554. Takahara K, Hoffman GG & Greenspan DS (1995) Complete structural organization of the human α1(V) collagen gene (COL5A1): divergence from the conserved organization of other characterized fibrillar collagen genes. Genomics 29: 588-597. Takahashi E, Hori T, O'Connell P, Leppert M & White R (1990) R-banding and nonisotopic in situ hybridization: precise localization of the human type II collagen gene (COL2A1). Hum Genet 86: 14-16. Temple IK (1989) Stickler’s syndrome. J Med Genet 26: 119-126. Terwilliger JD & Ott J (1994) Handbook of Human Genetic Linkage. John Hopkins University Press, Baltimore and London. Thalmann I (1993) Collagen of accessory structures of organ of Corti. Connect Tissue Res 29: 191203. Thalmann I, Thallinger G, Comegys TH & Thalmann R (1986) Collagen - the predominant protein of the tectorial membrane. ORL J Otorhinolaryngol Relat Spec 48: 107-115. Thalmann I, Thallinger G, Crouch EC, Comegys TH, Barrett N & Thalmann R (1987) Composition and supramolecular organization of the tectorial membrane. Laryngoscope 97: 357-367. Thomas DC, Kunkel TA, Casna NJ, Ford JP & Sancar A (1986) Activities and incision patterns of ABC excinuclease on modified DNA containing single-base mismatches and extrahelical bases. J Biol Chem 261: 14496-14505. Tiller GE, Warman ML, Gong Y, Knoll JHM, Mayne R & Brewton RG (1998) Physical and linkage mapping of the gene for the alpha-3 chain of type IX collagen, COL9A3, to human chromosome 20q13.3. Cytogenet Cell Genet 81: 205-207. Uitto J (1979) Collagen polymorphism: isolation and partial characterization of α1(I)-trimer molecules in normal human skin. Arch Biochem Biophys 192: 371-379. Vandenberg P, Khillan JS, Prockop DJ, Helminen H, Kontusaari S & Ala-Kokko L (1991) Expression of a partially deleted gene of human type II procollagen (COL2A1) in transgenic mice produces a chondrodysplasia. Proc Natl Acad Sci USA 88: 7640-7644. Varlotta GP, Brown MD, Kelsey JL & Golden AL (1991) Familial predisposition for herniation of a lumbar disc in patients who are less than twenty-one years old. J Bone Joint Surg [Am] 73: 124-128. Vasios G, Nishimura I, Konomi H, van der Rest M, Ninomiya Y & Olsen BR (1988) Cartilage type IX collagen-proteoglycan contains a large amino-terminal globular domain encoded by multiple exons. J Biol Chem 263: 2324-2329. Vaughan L, Mendler M, Huber S, Bruckner P, Winterhalter KH, Irwin MI & Mayne R (1988) DPeriodic distribution of collagen type IX along cartilage fibrils. J Cell Biol 106: 991-997. 71 Videman T, Leppävuori J, Kaprio J, Battié MC, Gibbons LE, Peltonen L & Koskenvuo M (1998) Intragenic polymorphisms of the vitamin D receptor gene associated with intervertebral disc degeneration. Spine 23: 2477-2485. Vikkula M, Mariman ECM, Lui VCH, Zhidkova NI, Tiller GE, Goldring MB, van Beersum SEC, de Waal Malefijt MC, van den Hoogen FHJ, Ropers H-H, Mayne R, Cheah KSE, Olsen BR, Warman ML & Brunner HG (1995) Autosomal dominant and recessive osteochondrodysplasias associated with the COL11A2 locus. Cell 80: 431-437. Vikkula M, Metsäranta M & Ala-Kokko L (1994) Type II collagen mutations in rare and common cartilage diseases. Ann Med 26: 107-114. Vintiner GM, Temple IK, Middleton-Price HR, Baraitser M & Malcolm S (1991) Genetic and clinical heterogeneity of Stickler syndrome. Am J Med Genet 41: 44-48. Vissing H, D’Alessio M, Lee B, Ramirez F, Godfrey M & Hollister DW (1989) Glycine to serine substitution in the triple helical domain of pro-alpha 1(II) collagen results in a lethal perinatal form of short-limbed dwarfism. J Biol Chem 264: 18265-18267. Vuorio E & Crombrugghe B (1990) The family of collagen genes. Annu Rev Biochem 59: 837872. Vuoristo M, Pihlajamaa T, Vandenberg P, Prockop DJ & Ala-Kokko L (1995) The human COL11A2 gene structure indicates that the gene has not evolved with the genes for the major fibrillar collagens. J Biol Chem 270: 22873-22881. Wagner R, Debbie P & Radman M (1995) Mutation detection using immobilized mismatch binding protein (MutS). Nucleic Acid Res 23: 3944-3948. Warman M, Kimura T, Myragaki Y, Castagnola P, Tamei H, Iwata K & Olsen BR (1993a) Monoclonal antibodies against two epitopes in the human α1(IX) collagen chain. Matrix 13: 149-153. Warman ML, McCarthy MT, Perälä M, Vuorio E, Knoll JHM, McDaniels CN, Mayne R, Beier DR & Olsen BR (1994) The genes encoding alpha-2(IX) collagen (COL9A2) map to human chromosome 1p32.3-p33 and mouse chromosome 4. Genomics 23: 158-162. Warman ML, Tiller GE & Griffith AJ (1998) Reply to Shanske et al. (letter). Am J Hum Genet 63: 1559-1561. Warman ML, Tiller GE, Polumbo PA, Seldin MF, Rochelle JM, Knoll JHM, Cheng S-D & Olsen BR (1993b) Physical and linkage mapping of the human and murine genes for the alpha-1 chain of type IX collagen (COL9A1). Genomics 17: 694-698. Watanabe H, Kimata K, Line S, Strong D, Gao LY, Kozak CA & Yamada Y (1994) Mouse cartilage matrix deficiency (cmd) caused by a 7 bp deletion in the aggrecan gene. Nat Genet 7: 154-157. Watanabe H, Nakata K, Kimata K, Nakanishi I & Yamada Y (1997) Dwarfism and age-associated spinal degeneration of heterozygote cmd mice defective in aggrecan. Proc Natl Acad Sci USA 94: 6943-6947. Weis MA, Wilkin DJ, Kim HJ, Wilcox WR, Lachman RS, Rimoin DL, Cohn DH & Eyre DR (1998) Structurally abnormal type II collagen in a severe form of Kniest dysplasia caused by an exon 24 skipping mutation. J Biol Chem 273: 4761-4768. Weishaupt D, Zanetti M, Hodler J & Boos N (1998) MR imaging of the lumbar spine: prevalence of intervertebral disc extrusion and sequestration, nerve root compression, end plate abnormalities, and osteoarthritis of the facet joint in asymptomatic volunteers. Radiology 209: 661-666. Werle E, Schneider C, Renner M, Volker M & Fiehn W (1994) Convenient single-step, one tube purification of PCR products for direct sequencing. Nucleic Acid Res 22: 4354-4355. Wilkin DJ, Mortier GR, Johnson CL, Jones MC, de Paepe A, Shohat M, Wildin RS, Falk RE & Cohn DH (1998) Correlation of linkage data with phenotype in eight families with Stickler syndrome. Am J Med Genet 80: 121-127. Williams CJ, Ganguly A, Considine E, McCarron S, Prockop DJ, Walsh-Vockley C & Michels VV (1996) A-2 → G transition at the 3’ acceptor splice site of IVS17 characterizes the COL2A1 gene mutation in the original Stickler syndrome kindred. Am J Med Genet 63: 461-467. 72 Winter RM, Baraitser M, Laurence KM, Donnai D & Hall CM (1983) The WeissenbacherZweymüller, Stickler, and Marshall syndromes: further evidence for their idenetity. Am J Med Genet 16: 189-199. Wordsworth P, Ogilvie D, Priestley L, Smith R, Wynne-Davies R & Sykes B (1988) Structural and segregation analysis of the type II collagen gene (COL2A1) in some heritable chondrodysplasias. J Med Genet 25: 521-527. Wu J-J & Eyre DR (1995) Structural analysis of cross-linking domains in cartilage type XI collagen. J Biol Chem 270: 18865-18870. Wu J-J, Woods PE & Eyre DR (1992) Identification of cross-linking sites in bovine cartilage type IX collagen reveals an antiparallel type II-type IX molecular relationship and type IX to type IX bonding. J Biol Chem 267: 23007-23014. Yada T, Suzuki S, Kobayashi K, Kobayashi M, Hoshino T, Horie K & Kimata K (1990) Occurrence in chick embryo vitreous humor of a type IX collagen proteoglycan with an extraordinarily large chondroitin sulfate chain and short alpha 1 polypeptide. J Biol Chem 265: 6992-6999. Yang SS, Chen H, Williams P, Cacciarelli A, Mistra RP & Bernstein J (1980). Spondyloepiphyseal dysplasia congenita. A comparative study of chondrocytic inclusions. Arch Pathol Lab Med 104: 208-211. Yoo TJ, Cho H & Yamada Y (1991) Hearing impairment in mice with the cmd/cmd (cartilage matrix deficiency) mutant gene. Ann N Y Acad Sci 630: 265-267. Youil R, Kemper BW & Cotton RGH (1995) Screening for mutations by enzyme mismatch cleavage with T4 endonuclease VII. Proc Natl Acad Sci USA 92: 87-91. Zhidkova NI, Brewton RG & Mayne R (1993) Molecular cloning of PARP (proline/arginine-rich protein) from human cartilage and subsequent demonstration that PARP is a fragment of the NH2-terminal domain of the collagen α2(XI) chain. FEBS Lett 326: 25-28. Zhidkova NI, Justice SK & Mayne R (1995) Alternative mRNA processing occurs in the variable region of the pro-α1(XI) and pro-α2(XI) collagen chains. J Biol Chem 270: 9486-9493. Zlotogora J, Sagi M, Schuper A, Leiba H & Merin S (1992) Variability of Stickler syndrome. Am J Med Genet 42: 337-379.