EMQN best practice guidelines for the laboratory diagnosis of osteogenesis imperfecta

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Osteogenesis imperfecta (OI) comprises a group of inherited disorders characterized by bone fragility and increased susceptibility to fractures. Historically, the laboratory confirmation of the diagnosis OI rested on cultured dermal fibroblasts to identify decreased or abnormal production of abnormal type I (pro)collagen molecules, measured by gel electrophoresis. With the discovery of COL1A1 and COL1A2 gene variants as a cause of OI, sequence analysis of these genes was added to the diagnostic process. Nowadays, OI is known to be genetically heterogeneous. About 90% of individuals with OI are heterozygous for causative variants in the COL1A1 and COL1A2 genes. The majority of remaining affected individuals have recessively inherited forms of OI with the causative variants in the more recently discovered genes CRTAP, FKBP10, LEPRE1,PLOD2, PPIB, SERPINF1, SERPINH1 and SP7, or in other yet undiscovered genes. These advances in the molecular genetic diagnosis of OI prompted us to develop new guidelines for molecular testing and reporting of results in which we take into account that testing is also used to ‘exclude’ OI when there is suspicion of non-accidental injury. Diagnostic flow, methods and reporting scenarios were discussed during an international workshop with 17 clinicians and scientists from 11 countries and converged in these best practice guidelines for the laboratory diagnosis of OI.


Classification of osteogenesis imperfecta

Osteogenesis imperfecta (OI) comprises a heterogeneous group of disorders characterized by susceptibility to bone fractures with severity that ranges from death in the perinatal period to subtle increase in fracture frequency and in almost all cases presumed or proven defects in type I (pro)collagen biosynthesis.1 In 1979, David Sillence developed a four-type classification, which is still in use for classification according to clinical/radiological features: OI type I (mild OI with bone fragility and blue sclerae), II (perinatal lethal), III (progressive deforming) and IV (normal sclerae and mild deformity).2, 3 Dominant COL1A1/2 variants appeared to be causative in the majority of OI types. In 2004, OI types V and VI were added to this classification because of specific clinical/radiological and/or histological features, absence of abnormalities of type I (pro)collagen synthesis or structure on gel electrophoresis and absence of causative variants in the COL1A1/2 genes.4, 5 With the discovery of rare recessive genetic causes of OI (see Table 1), it was proposed to extend the classification with OI types VII and VIII.6 However, the classification and subdivision into different types of OI is still under discussion1 because the phenotypic spectrum that results from mutations in some of these genes is almost as broad as that with mutations in type I collagen genes. There is also debate as to whether Bruck syndrome type I7 and II,8 characterized clinically by bone fragility and congenital contractures of the large joints, should be classified as a type of OI.

Table 1 Genes in which sequence variants cause OI

Biosynthesis of type I collagen

Most individuals affected with OI are heterozygous for a causative variant in either of the two genes, COL1A1 or COL1A2, which encode the proα1(I) and proα2(I) chains of type I procollagen, respectively. Type I collagen is the major structural protein in bone, tendon and ligament. Recently, rare recessive genetic causes of OI have been described and, in all but one, the identified genes encode proteins involved in the biosynthesis of type I procollagen (Figure 1, Tables 1 and 2).9, 10

Figure 1

Critical steps in collagen type I biosynthesis and indication of genes known to be involved in OI. Type I collagen is the major structural protein in bone, tendon and ligament. It is first synthesized in the rough endoplasmic reticulum (rER) as type I procollagen, containing C- and N-terminal propeptides. In the rER, the two α1(I)-collagen chains encoded by COL1A1 and the one α2(I)-collagen chain encoded by COL1A2 comprising predominantly Gly-X-Y triplets, align and assemble in the C- to-N direction to form a triple helix. During folding, collagen is modified by, among others, specific enzymes that hydroxylate lysine and proline residues and glycosylate hydroxylysyl residues. This process is called post-translational modification and it stops when triple helix assembly is complete. The CRTAP/P3H1/CyPB complex encoded by the CRTAP, LEPRE1 and PPIB genes, is responsible for the 3-hydroxylation of P986 (p.P1164 counting from the methionine that initiates translation) but will most likely also act as a cis-trans isomerase and a molecular chaperone. FKBP65 encoded by FKBP10 also acts as a molecular chaperone for type I procollagen. The protein product of PLOD2 (procollagen-lysine, 2-oxoglutarate 5-dioxygenase 2) hydroxylates telopeptide lysines in the rER. HSP47 encoded by SERPINH1 is thought to maintain the stability of the triple helix. After folding, the procollagen molecules are transported through the Golgi apparatus and plasma membrane (PM) into the extracellular matrix (ECM) where cleavage of the N-and C-terminal propeptides occurs and collagen molecules aggregate to form fibrils.

Table 2 Characteristics of recessive OI-related genes

Genes, proteins and causative variants

Autosomal dominant OI

The most common form of OI in most populations is OI type I. Cultured dermal fibroblasts from affected individuals produce about half the normal amount of type I procollagen molecules, which have normal structure. OI type I usually results from variants in one COL1A1 allele (frameshift, nonsense and splice-site alterations) that lead to mRNA instability and haploinsufficiency. In a small subset of individuals with OI type I, substitutions for glycine by small amino acids (cysteine, alanine and serine) near the amino terminal ends of the triple-helical domains of either COL1A1 or COL1A2 are found. In contrast, OI types II–IV are usually caused by sequence variants in either COL1A1 or COL1A2 that result in substitutions for glycine residues in the uninterrupted Gly-X-Y triplet repeat of the 1014-residue triple-helical domains encoded by each gene. Less common causative variants include splice-site alterations, variants in the carboxyl-terminal propeptide coding-domains or insertion/deletion events that lead to in-frame sequence alterations. Most of these variants result in synthesis of abnormal type I procollagen molecules characterized by post-translational over-modification of the triple-helical domain, which results in alterations visible by SDS-polyacrylamide gel electrophoresis. Loss of expression of either gene because of large-scale deletions appears to be rare.11, 12, 13, 14, 15 More than 1000 distinct variants in the COL1A1 and COL1A2 genes have been identified that cause OI (R Dalgleish: Osteogenesis Imperfecta Variant Database (https://oi.gene.le.ac.uk, accessed 3 May 2011).16, 17

Autosomal recessive OI including Bruck syndrome

In the last 5 years, candidate–gene approaches have identified several loci in which causative variants have been identified which result in the long-sought causes for recessively inherited forms of OI (see Figure 1, Table 2). We classify these genes in four groups—(i) one in which the genes encode proteins that contribute to the initial phase of chain recognition and propagation of molecular folding (CRTAP, LEPRE1 and PPIB)18, 19, 20, 21, 22, 23, 24, 25, 26 the second in which the genes encode proteins involved in the final quality control of type I procollagen (FKBP1027, 28, 29 and SERPINH130), the third, which involves a gene encoding proteins involved in late modification and crosslink formation (PLOD28, 31) and the fourth group, which involves recently recognized genes encoding proteins involved in bone cell differentiation (SP732 and possibly SERPINF133).

Reasons for referral


Prenatal ultrasounds showing abnormalities suggestive of OI (diminished mineralization of skull, platyspondyly or bowing, shortening and/or fractures of long bones) are an important reason for referral for molecular diagnostics of OI.


Radiographs at birth suggestive of OI, recurrent and/or unexplained fractures with or without suspicion of non-accidental injury (NAI), primary (idiopathic) low bone mass, preferably with exclusion of secondary causes, a family history of OI and request for confirmation of the clinical diagnosis are all reasons for referral for molecular diagnostics of OI. However, in some cases dentinogenesis imperfecta or even blue sclerae might be the only reason for referral. As such, physicians from many specialties (gynaecologist, paediatrician, orthopaedic surgeon, clinical geneticist, general practitioner, dentist, ear nose throat specialist, endocrinologist, internist and ophthalmologist) might refer a patient for molecular analysis. Depending on the age of presentation, OI can be difficult to distinguish from some other genetic conditions, for example, Ehlers–Danlos syndrome arthrochalasis type (former EDS VIIA and B), isolated dentinogenesis imperfecta, blue sclerae and corneal fragility, hypophosphatasia, and non-genetic causes of fractures including NAI and idiopathic juvenile osteoporosis.2, 34, 35, 36

Non-accidental injury

Many referrals for OI diagnostics occur in the context of suspected NAI in an attempt to exclude a genetic cause of fractures. Fractures resulting from NAI occur in 24 per 10 000 children under 3 years of age whereas the OI prevalence is 1 per 10 000–20 000.34 The incidence of OI among children evaluated for NAI is 2–5%.34 Differentiation is aided by an experienced clinician and radiologist familiar with OI36 as the nature and localization of fractures in OI and NAI can often be distinguished.37 However, because injuries may involve infants before many of the clinical features of OI are apparent, laboratory diagnostics for OI can certainly be helpful in this differentiation.

Materials and methods

A group of clinicians and scientists involved in OI diagnostics met on 28–29 June 2010 at a workshop in Amsterdam, the Netherlands, to formulate Best Practice Guidelines for the molecular genetic diagnosis of OI supported by the European Molecular Genetics Quality Network (EMQN).


Discussions focussed on diagnostic flow, methodologies, interpretation of results and reporting. Consensus guidelines were established.


The diagnostic flow

The ‘traditional’ way to establish or confirm the diagnosis of OI is based on studies of collagens synthesized by cultured dermal fibroblasts. Previous studies35 demonstrated that either quantitative or qualitative alterations can be identified in about 90%38 of individuals with clinically confirmed OI. Biochemical analysis will separate individuals with quantitative defects (OI type I), from those with qualitative defects (OI types II–IV) because of causative variants in the COL1A1/2, CRTAP, LEPRE1, PPIB genes and those with no abnormalities detected. Electrophoretic analysis of type I procollagen may also identify other disorders that can mimic some aspects of OI: EDS kyphoscoliotic type (type VIA), EDS arthrochalasia type (types VIIA and VIIB) and EDS dermatosparaxis type (type VIIC).11 Also, cultured fibroblasts provides a resource for the analysis of RNA splicing and unclassified variants. However, biochemical analysis will not identify some quantitative defects of type I procollagen, certain causative variants that alter sequences in some coding regions of the COL1A1/COL1A2 genes and recessive forms of OI (including Bruck syndrome) that result from variants in FKBP10, PLOD2, SERPINF1, SERPINH1 or SP7. Furthermore, prenatal diagnosis by biochemical analysis is only possible in chorionic villus cells and is effective with qualitative alterations9 but unsuitable for quantitative defects and delays time of diagnosis by 2–4 weeks compared with genetic analysis.

In contrast, direct genomic analysis (sequencing) of the known genes should identify causative variants in >95% of affected individuals in most populations.39, 40 Next generation sequencing has gained importance in the laboratory diagnosis of OI – in part because of shorter time to diagnosis and in part because of the added value of the information as well as reduced costs, which is important for the precise determination of recurrence risk (autosomal dominant versus recessive), prenatal diagnosis and pre-implantation genetic diagnosis.

Given these considerations and current facilities, the consensus of the EMQN Best Practice in OI meeting was to initiate laboratory-based diagnostic studies with direct genomic sequencing of the type I procollagen genes, COL1A1 and COL1A2. The approach to diagnosis is detailed in Figure 2. It was agreed that the ‘traditional’ approach can still be used in the context in which genomic DNA sequencing is unavailable or the financial barriers are high. Moreover, analysis of proteins and mRNA/cDNA from cultured fibroblasts remain valuable tools for follow-up studies.

Figure 2

Preferred diagnostic flow in OI. The approach to diagnosis is designed to maximize the likelihood that causative variants will be identified in all affected individuals or assign those without causative variants to research pools. This flow assumes that the clinical diagnosis of OI is well established according to the traditional diagnostic criteria. With clear evidence of OI from radiological and clinical examination, further analysis should proceed according to the proposed strategy. Functional analysis consists of analysis of proteins and mRNA/cDNA from cultured fibroblasts and also includes COL1A1 null allele testing in certain selected cases.

Explanation of diagnostic work flow

Sequencing of all type I procollagen gene exons

Procollagen type I gene sequencing should identify causative variants in 90% of affected individuals,39, 40 provided that the clinical diagnosis of OI is accurate. In some cases a follow-up study is needed to determine whether a variant is causative. This will often include genetic studies in the parents with correlation to the phenotype observed in the parent, or analysis of mRNA splicing and protein-based biochemical studies on cultured dermal fibroblasts.

If no causative variant in the COL1A1/2 genes is identified by sequence analysis, the next step is to determine if a deletion or duplication of some or all of the coding regions of either gene has occurred. Strategies such as array-based analysis, MLPA or qPCR if properly validated are considered equivalent by the working group in their detection of such alterations. From currently available data in the represented laboratories, the added causative variants expected from this approach should be about 1–2%. In case of OI types II–IV, after identifying the causative variant in the index patient, determination of parental mosaicism by sequence analysis of DNA from blood from each parent will provide data for genetic counselling with respect to recurrence risk and care in subsequent pregnancies.

Re-review of clinical data and the question of NAI

When no causative COL1A1/2 variant is found, clinical priorities should be re-considered. Failure to find a causative variant occurs if there is technical failure, or if no causative variant is present in these genes (because of causative variants in other (un)known genes or because the patient does not have OI). Therefore, referring physicians should be encouraged to provide a completed clinical checklist (Supplementary Table 1) and X-rays of the patient. This clinical/radiological information should be reviewed by a clinical geneticist or a clinician with experience in OI. This can help to determine the likelihood of OI in the particular patient. With clear evidence of OI, further analysis should proceed (Figure 2).

However, if the primary reason for genetic study is to identify children with OI among the larger group suspected for NAI, analysis can reasonably stop after COL1A1/2 sequencing unless there is a strong suggestion of consanguinity or recessive inheritance. Justification of this decision rests on the following considerations. First, previous studies indicate that fewer than 5% of infants studied for suspicion of NAI are found to have OI by biochemical or DNA-based studies.34 Second, DNA-based analysis will identify a causative variant in >90% of all individuals with OI39, 40 so that the remaining risk that an infant has OI, will be about 0.5%. Third, at present all infants with recessive OI have obvious radiographic abnormalities fitting a diagnosis of OI and not of NAI.

Identification and characterization of causative variants in autosomal recessive OI

Variants in the genes causing recessive OI are estimated to account for about 5 or 6% of individuals with OI. This represents the pooled estimates from all the laboratories represented at the workshop. Although laboratory context and clinical criteria may in some cases require otherwise, the preferred strategy is to analyse all genes at the same time to minimize turnaround time. If no, or only one, causative variant is identified by sequence analysis, the next step is to determine by array-based analysis, MLPA or qPCR if a deletion or duplication of some or all of the coding regions of either allele has occurred. Once recessive causative variants are identified, parental confirmation of carrier status should be completed, first to confirm that the causative variants in the index case are inherited in trans and, second, to exclude the possibility of uniparental disomy in the case of homozygosity in the infant.

Analysis of proteins and mRNA/cDNA from cultured fibroblasts (functional analysis)

By following the guidelines to this point, virtually all causative variants in type I procollagen genes and in the recessive OI-related genes will have been identified. However, in some cases analysis of proteins and mRNA/cDNA from cultured fibroblasts can have an additive value. First of all, mRNA/cDNA analysis provides a tool for studying the effect of unclassified variants suspected to alter splicing. Moreover, this approach can unravel the effect of deep intronic variants that alter the mRNA sequences usually by conversion of cryptic exons to active exons and which would not be detected by gDNA sequencing. In these cases, biochemical analysis of type I procollagen chains can detect quantitative defects if the new exon results in introduction of a premature stop codon and nonsense-mediated mRNA decay, or qualitative defects if the mRNA is stable and translated into an abnormal protein. When OI type I is suspected, but genomic DNA sequencing is unavailable or too costly, COL1A1 null-allele14 testing on cDNA can be used to confirm the diagnosis. However, this approach relies on the availability of informative markers and will not lead to the identification of the disease-causing variant.

Analysis of remaining samples

Some diagnostic laboratories maintain research arms and the identification of the additional OI-related genes has profited from the repositories of cells and DNA samples from individuals with OI because of unknown genetic causes. This practice should continue and cells and DNA samples should be banked for future analysis. If the diagnostic laboratory does not maintain such a resource, banking with ones that do, should be considered.

Laboratory diagnosis of OI

Molecular analysis for OI

Molecular analysis for OI includes sequencing or mutation scanning and deletion/duplication testing for COL1A1 and COL1A2, followed by sequencing of recessive OI-related genes (see Table 1). Preferred material for testing is genomic DNA from blood, but other sources can be used as well (see Tables 3a and b). For general issues regarding sample labelling and identification, sequence analysis and interpretation see ‘Practice guidelines for Sanger Sequencing Analysis and Interpretation’ (http://www.cmgs.org/BPGs/pdfs%20current%20bpgs/Sequencingv2.pdf).

Table 3a Postnatal diagnostics for OI
Table 3b Prenatal and preimplantation genetic diagnosis for OI

gDNA and cDNA sequencing

Current practices in sequencing of the type I collagen genes differ among laboratories in that some use exon-by-exon amplification followed by sequence determination (Supplementary Appendix Tables 3A and B) and others use a multi-exon substrate for analysis. If properly validated, both will provide the same mutation capture probability and their use should be determined by local preferences. To identify splice variants, primer sequences for PCR used for direct sequencing should be designed far enough from intron–exon boundaries to allow reading of the branch sites, consensus splice donor and acceptor sites or UTR sequences of acceptable quality. With regard to sequence analysis of cDNA, large fragments should be analysed to allow detection of multi-exon deletions, because these could be missed when primers are located close to the exon junctions at multiple sites. The analysis of cDNA from fibroblasts is warranted when an unknown variant is found that might affect splicing. In addition, cDNA sequence analysis may detect null-alleles without a known cause (eg, an unknown variant in the promoter region) if care is taken to analyse regions in which coding sequence heterozygosity is known.

Quantitative analysis

Quantitative analysis by MLPA (kits for COL1A1 and COL1A2 have been designed by MRC-Holland, available at http://www.mlpa.com) and qPCR is particularly important in cases without a detected molecular cause in which only genomic DNA is available and without heterozygous polymorphic variants detected by sequencing. Recently, complete COL1A1 allele deletions have been reported to cause OI type I.13 For reliable quantitative testing (MLPA/qPCR) patient and control materials from the same source (eg, blood or fibroblasts) should be used for comparison and the same DNA purification protocol should be used for all samples within a test series.

Protein analysis

Protein analysis of type I (pro)collagen (Supplementary Appendix Figures 3A–D) is used to detect quantitative and qualitative changes. The method used for this analysis is based on in vitro labelling of collagen in cultured fibroblasts, followed by electrophoresis on 2 M urea SDS-PAGE gels (the 2 M urea enhances chain separation) and autoradiography.41 The analysis of procollagens is achieved by omitting the pepsin digestion step from the collagen protocol. Procollagen electrophoresis enhances detection sensitivity of quantitative type I (pro)collagen defects (OI type I), visualizes defects in type I (pro)collagen located in the N-terminal region of the type I collagen triple helix more clearly and distinguishes between EDS VIIC and EDS VIIA and B (if samples are analysed after labelling in the presence and absence of dextran sulphate to enhance proteolytic processing).42

Prenatal diagnosis

Prenatal diagnosis is possible in case of identification of known disease-causing variant(s) both on genomic DNA extracted from chorionic villus sample (CVS) cells and amniocytes. ‘Testing for Maternal Cell Contamination (MCC) in Prenatal Samples for Molecular Studies’ (http://www.cmgs.org/BPGs/pdfs%20current%20bpgs/MCC_08.pdf) should be applied. In those rare instances when post-translational over-modification of (pro)collagen type I is visible in, for example, cells from an affected sibling but no disease-causing variant(s) have been detected in the genes involved in OI, electrophoresis of type I (pro)collagen from cultured CVS cells can be used for prenatal diagnosis. Amniocytes are good sources of DNA but they do not make type I procollagen in sufficient abundance to permit prenatal diagnosis.

Interpretation of performed diagnostics

For the interpretation of an observed sequence variant it is essential to establish the causal role of the variant in the pathogenesis of the disease. Textboxes 1 and 2 include descriptions of variants in the genes involved in OI that are likely to be pathogenic or that should be considered as unclassified variants.


General information on requirements for variant reporting can be found in the OECD Guidelines for Quality Assurance in Molecular Genetic Testing (http://www.OECD.org/dataoecd/43/6/38839788.pdf) and in the guidelines issued by the Swiss Medical Genetics Society (http://sgmg.ch/user_files/images/SGMG_Reporting_Guidelines.pdf).

Reporting scenarios

Finding a causative variant in the COL1A1/COL1A2 genes in an affected index case

The report should state that a causative variant has been detected and that this confirms the clinical diagnosis. The report should include a description of the reason why a particular variant is considered causative. Determination of the parental origin of the detected variant(s) should be advised. Testing of relatives at risk should be offered in conjunction with appropriate counselling.

In the case of severe/lethal OI because of a causative variant in COL1A1 or COL1A2, the measured recurrence risk is 2% after the birth of one affected child. The recurrence risk is increased after the birth of two affected individuals, presumably because the proportion of germ cells that carry the mutation is higher.43 This information may be mentioned in the results letter. If parental mosaicism can be demonstrated in the father, the referring clinician could be encouraged to request a sperm sample from the father to clarify the risk.

When the referring physician is not a clinical geneticist, it is recommended that the patient be referred to a clinical genetics centre for counselling. Referral to OI centres for therapy can be proposed if available.

Not finding a causative variant in COL1A1 and COL1A2 genes in an affected index case

If no causative variant is detected in the COL1A1 and COL1A2 genes after gDNA analysis and screening for large gene deletions (eg, MLPA), an interim report can be made with the recommendation for review of the original patient diagnosis (detailed clinical information, eg, with use of the clinical checklist, radiographs, contact with the referring physician (see Supplementary Appendix Table 1)). This review of the clinical diagnosis should involve a clinician with expertise in diagnosis and classification of OI. The outcome of this review might indicate the desirability for testing of additional OI genes and cDNA and protein analysis of type I (pro)collagen. If applicable, a new request for additional testing should be sent by the referring physician to the laboratory. Laboratories that do not offer analysis of the recessive genes should suggest further analysis in another laboratory.

In the case of doubtful pathogenicity of the identified variant, the ‘Practice guidelines for the Interpretation and Reporting of Unclassified Variants (UV's) in Clinical Molecular Genetics’ (http://www.cmgs.org/BPGs/pdfs%20current%20bpgs/UV%20GUIDELINES%20\ratified.pdf) should be applied. If the genetic testing procedure has identified an unclassified variant as the only sequence change, this should be reported as such. However, the report should clearly state that the clinical significance of the variant is unknown and that its identification does not provide an explanation for the clinical phenotype of the patient.

Finding causative variants in the CRTAP, LEPRE1, PPIB, FKBP10, SERPINF1, SERPINH1, PLOD2, SP7 genes in an affected index case

The final report should state that causative variants have been detected. It is necessary to investigate the carrier status of the parents and siblings in order to determine whether a variant is causative. Testing of relatives at risk may be offered in conjunction with appropriate counselling. Such testing might be useful for prenatal diagnosis.

Finding one causative variant in the CRTAP, LEPRE1, PPIB, FKBP10, SERPINF1, SERPINH1, PLOD2, SP7 genes in an affected index case

When one causative recessive variant has been detected, it cannot be excluded that a second causative variant has been missed, for example when it concerns a deep intronic variant. Dependent on the laboratory, a second interim report can be made indicating the desirability for cDNA and protein analysis of type I (pro)collagen in the case of one causative variant in the CRTAP, LEPRE1 or PPIB genes. When these additional tests are not informative or cannot be performed in the laboratory, the final report should state that it is not possible to confirm the clinical diagnosis OI by biochemical and/or molecular testing.

Not finding causative variants in the CRTAP, LEPRE1, PPIB, FKBP10, SERPINF1, SERPINH1, PLOD2, SP7 genes in an affected index case

In the case of doubtful pathogenicity of the identified variants, the same procedure as described above for the COL1A1 and COL1A2 genes should be followed. In the case where no causative variants in the genes involved in recessive OI have been found, the final report should state that it is not possible to confirm the clinical diagnosis OI by biochemical and/or molecular testing.

Not finding causative variant(s) in the genes known for autosomal dominant and autosomal recessive OI: type I (pro)collagen electrophoresis

Reports of these studies are necessarily more descriptive than the DNA-based results. They should list the types of genetic alterations that could not be identified. When low production or post-translational over-modification of type I (pro)collagen is observed, the diagnosis of OI can be confirmed and in the case of over-modification of type I (pro)collagen, prenatal diagnosis on chorionic villus cells is possible. In reports concerning cells and samples with no molecular and/or biochemical diagnosis of OI, it should be stated that it is not possible to confirm the clinical diagnosis OI.

Prenatal or preimplantation genetic diagnosis

Prenatal or preimplantation genetic diagnosis with the intention of terminating a pregnancy or not selecting embryos carrying the causative variant(s) is possible in the case of identification of known disease-causing variant(s). This service should only be offered in a clinical genetics service and must be accompanied by appropriate genetic counselling. Requests for prenatal or preimplantation diagnosis should always be referred and announced in advance to a clinical genetics service. In addition, the original result letter of the laboratory that identified the causative variant should accompany the request.


Best practice guidelines have been established for the molecular genetic diagnosis of OI. The most noteworthy issue is that molecular analysis of the COL1A1/2 genes is recommended as the starting point in the diagnostic flow as opposed to protein analysis. It is to be expected that molecular genetic testing in OI will only gain in importance as new OI-genes are discovered and with the development of new technologies. However, in certain selected cases protein analysis will remain important.


  1. 1

    van Dijk FS, Pals G, van Rijn RR, Nikkels PGJ, Cobben JM : Classification of osteogenesis imperfecta revisited. Eur J Med Genet 2010; 53: 1–5.

  2. 2

    Byers PH, Krakow D, Nunes ME, Pepin M : Genetic evaluation of suspected osteogenesis imperfecta (OI). Genet Med 2006; 8: 383–388.

  3. 3

    Sillence DO, Senn A, Danks DM : Genetic heterogeneity in osteogenesis imperfecta. J Med Genet 1979; 16: 101–116.

  4. 4

    Glorieux FH, Rauch F, Plotkin H et al: Type V osteogenesis imperfecta: a new form of brittle bone disease. J Bone Miner Res 2000; 15: 1650–1658.

  5. 5

    Glorieux FH, Ward LM, Rauch F, Lalic L, Roughly PJ, Travers R : Osteogenesis imperfecta type VI: a form of brittle bone disease with mineralization defect. J Bone Miner Res 2002; 17: 30–37.

  6. 6

    Rauch F, Glorieux FH : Osteogenesis imperfecta. Lancet 2004; 363: 1377–1385.

  7. 7

    Breslau-Siderius EJ, Engelbert RH, Pals G, van der Sluijs JA : Bruck syndrome: a rare combination of bone fragility and multiple congenital joint contractures. J Pediatr Orthop B 1998; 7: 35–38.

  8. 8

    Ha-Vinh R, Alanay Y, Bank RA et al: Phenotypic and molecular characterization of Bruck syndrome (osteogenesis imperfecta with contractures of the large joints) caused by recessive mutation in PLOD2. Am J Med Genet 2004; 131A: 115–120.

  9. 9

    Engel J, Prockop DJ : The zipper-like folding of collagen triple helices and the effects of mutations that might disrupt the zipper. Annu Rev Biophys Biophys Chem 1991; 20: 137–152.

  10. 10

    Byers PH, Wallis GA, Willing MC : Osteogenesis imperfecta: translation of mutation to phenotype. J Med Genet 1991; 28: 433–442.

  11. 11

    Steiner RD, Pepin MG, Byers PH : Osteogenesis imperfecta. Available at http://www.ncbi.nlm.nih.gov/bookshelf/br.fcgi?book=gene&part=oi. Accessed 3 May 2011.

  12. 12

    Willing MC, Pruchno CJ, Atkinson M, Byers PH : Osteogenesis imperfecta type I is commonly due to a COL1A1 null allele of type I collagen. Am J Hum Genet 1992; 51: 508–515.

  13. 13

    Willing MC, Deschenes SP, Scott DA et al: Osteogenesis imperfecta type I: molecular heterogeneity for COL1A1 null alleles of type I collagen. Am J Hum Genet 1994; 55: 638–647.

  14. 14

    Nuytinck L, Sayli BS, Karen W, De Paepe A : Prenatal diagnosis of osteogenesis imperfecta type I by COL1A1 null-allele testing. Prenat Diagn 1999; 19: 873–875.

  15. 15

    van Dijk FS, Huizer M, Kariminejad A et al: Complete COL1A1 allele deletions in osteogenesis imperfecta. Genet Med 2010; 12: 736–741.

  16. 16

    Dalgleish R : The human type I collagen mutation database. Nucleic Acids Res 1997; 25: 181–187.

  17. 17

    Dalgleish R : The human collagen mutation database 1998. Nucleic Acids Res 1998; 26: 253–255.

  18. 18

    Ishikawa Y, Wirz J, Vranka JA, Nagata K, Bächinger HP : Biochemical characterization of the prolyl 3-hydroxylase 1·cartilage-associated protein·cyclophilin B complex. J Biol Chem 2009; 284: 17641–17647.

  19. 19

    Barnes AM, Chang W, Morello R et al: Deficiency of cartilage-associated protein in recessive lethal osteogenesis imperfecta. N Engl JMed 2006; 355: 2757–2764.

  20. 20

    Morello R, Bertin TK, Chen Y et al: CRTAP is required for prolyl 3- hydroxylation and mutations cause recessive osteogenesis imperfecta. Cell 2006; 127: 291–304.

  21. 21

    Marini JC, Cabral WA, Barnes AM : Null mutations in LEPRE1 and CRTAP cause severe recessive osteogenesis imperfecta. Cell Tissue Res 2010; 339: 59–70.

  22. 22

    Cabral WA, Chang W, Barnes AM et al: Prolyl 3-hydroxylase 1 deficiency causes a recessive metabolic bone disorder resembling lethal/severe osteogenesis imperfecta. Nat Genet 2007; 39: 359–365.

  23. 23

    Willaert A, Malfait F, Symoens S et al: Recessive osteogenesis imperfecta caused by LEPRE1 mutations: clinical documentation and identification of the splice form responsible for prolyl 3-hydroxylation. J Med Genet 2009; 46: 233–241.

  24. 24

    van Dijk FS, Nesbitt IM, Zwikstra EH et al: PPIB mutations cause severe osteogenesis imperfecta. Am J Hum Gen 2009; 85: 521–527.

  25. 25

    Barnes AM, Carter EM, Cabral WA et al: Lack of cyclophilin B in osteogenesis imperfecta with normal collagen folding. N Engl J Med 2010; 362: 521–528.

  26. 26

    Pyott SM, Schwarze U, Christiansen HE et al: Mutations in PPIB (cyclophilin B) delay type I procollagen chain association and result in perinatal lethal to moderate osteogenesis imperfecta phenotypes. Hum Mol Genet 2011; 20: 1595–1609.

  27. 27

    Alanay Y, Avaygan H, Camacho N et al: Mutations in the gene encoding RER protein FKBP65 cause autosomal-recessive osteogenesis imperfecta. Am J Hum Genet 2010; 86: 551–559.

  28. 28

    Shaheen R, Al-Owain M, Sakati N, Alzayed ZS, Alkuraya FS : FKBP10 and Bruck syndrome. Phenotypic heterogeneity or call for reclassification? Am J Hum Genet 2010; 87: 306–307.

  29. 29

    Kelley BP, Malfait F, Bonafe L et al: Mutations in FKBP10 cause recessive osteogenesis imperfecta and Bruck syndrome. J Bone Miner Res 2011; 26: 666–672.

  30. 30

    Christiansen HE, Schwarze U, Pyott SM et al: Homozygosity for a missense mutation in SERPINH1, which encodes the collagen chaperone protein HSP47, results in severe recessive osteogenesis imperfecta. Am J Hum Genet 2010; 86: 389–398.

  31. 31

    van der Slot AJ, Zuurmond AM, Bardoel AFJ et al: Identification of PLOD2 as telopeptide lysyl hydroxylase, an important enzyme in fibrosis. J Biol Chem 2003; 278: 40967–40972.

  32. 32

    Lapunzina P, Aglan M, Temtamy S et al: Identification of a frameshift mutation in Osterix in a patient with recessive osteogenesis imperfecta. Am J Hum Genet 2010; 87: 110–114.

  33. 33

    Becker J, Semler O, Gilissen C et al: Exome sequencing identifies truncating mutations in human SERPINF1 in autosomal-recessive osteogenesis imperfecta. Am J Hum Genet 2011; 88: 362–371.

  34. 34

    Marlowe A, Pepin MG, Byers PH : Testing for osteogenesis imperfecta in cases of suspected non-accidental injury. J Med Gen 2002; 39: 382–386.

  35. 35

    Ablin DS, Greenspan A, Reinhart M, Grix A : Differentiation of child abuse from osteogenesis imperfecta. Am J Roentgenol 1990; 154: 1035–1046.

  36. 36

    Steiner RD, Pepin M, Byers PH : Studies of collagen synthesis and structure in the differentiation of child abuse from osteogenesis imperfecta. J Pediatr 1996; 128: 542–547.

  37. 37

    Bilo RAC, Robben SGF, van Rijn RR : Forensic Aspects of Paediatric Fractures; Differentiating Accidental Trauma from Child Abuse. 1st edn. Springer: Heidelberg, Dordrecht, London, New York, 2010.

  38. 38

    Wenstrup RJ, Willing MC, Starman BJ, Byers PH : Distinct biochemical phenotypes predict clinical severity in nonlethal variants of osteogenesis imperfecta. Am J Hum Genet 1990; 46: 975–982.

  39. 39

    Körkkö J, Ala-Kokko L, De Paepe A, Nuytinck L, Earley J, Prockop DJ : 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 1998; 62: 98–110.

  40. 40

    Sykes B, Ogilvie D, Wordsworth P et al: Consistent linkage of dominantly inherited osteogenesis imperfecta to the type I collagen loci: COL1A1 and COL1A2. Am J Hum Genet 1990; 46: 293–307.

  41. 41

    Steinmann B, Rao VH, Vogel A, Bruckner P, Gitzelmann R, Byers PH : Cysteine in the triple-helical domain of one allelic product of the α1(I) gene of type I collagen produces a lethal form of osteogenesis imperfecta. J Biol Chem 1984; 259: 11129–11138.

  42. 42

    Bateman JF, Golub SB : Assessment of procollagen processing defects by fibroblasts cultured in the presence of dextran sulfate. Biochem J 1990; 267: 573–577.

  43. 43

    Pyott SM, Schwarze U, Christiansen HE et al: Recurrence of perinatal lethal osteogenesis imperfecta in sibships: parsing the risk between parental mosaicism for dominant mutations and autosomal recessive inheritance. Genet Med 2011; 13: 125–130.

  44. 44

    Dalgleish R, Flicek P, Cunningham F et al: Locus Reference Genomic sequences: an improved basis for describing human DNA variants. Genome Med 2010; 2: 24.

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Funding for the Best Practice Meeting was provided by the European Molecular Genetics Quality Network (http://www.emqn.org).

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Correspondence to Gerard Pals.

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The authors declare no conflict of interest.

Additional information

This paper was presented at an EMQN Best Practice Meeting, 28–29 June 2010, Amsterdam, The Netherlands. Other participants at the EMQN Best Practice Meeting were Javier Garcia-Planells, Filomena Valentina Gentile, Anne-Sophie Lebre, Shirley McQuaid, Rebecca Pollitt, Agnieszka Rusinska, Thomas Schwarzbraun and Janneke Weiss. Affiliations can be found in Supplementary Appendix Table 2.

Supplementary Information accompanies the paper on European Journal of Human Genetics website

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van Dijk, F., Byers, P., Dalgleish, R. et al. EMQN best practice guidelines for the laboratory diagnosis of osteogenesis imperfecta. Eur J Hum Genet 20, 11–19 (2012) doi:10.1038/ejhg.2011.141

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  • EMQN
  • best practice
  • osteogenesis imperfecta
  • type I (pro)collagen
  • diagnosis
  • reporting

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