1. Genetics and Genomics
  2. Medicine

Tendon and motor phenotypes in the Crtap-/- mouse model of recessive osteogenesis imperfecta

  1. Matthew William Grol  Is a corresponding author
  2. Nele A Haelterman
  3. Joohyun Lim
  4. Elda M Munivez
  5. Marilyn Archer
  6. David M Hudson
  7. Sara F Tufa
  8. Douglas R Keene
  9. Kevin Lei
  10. Dongsu Park
  11. Cole D Kuzawa
  12. Catherine G Ambrose
  13. David R Eyre
  14. Brendan H Lee  Is a corresponding author
  1. Department of Molecular and Human Genetics, Baylor College of Medicine, United States
  2. Department of Orthopaedics and Sports Medicine, University of Washington, United States
  3. Shriners Hospital for Children, United States
  4. Department of Orthopaedic Surgery, UT Health Sciences Center, United States
https://doi.org/10.7554/eLife.63488
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Cite this article
  1. Matthew William Grol
  2. Nele A Haelterman
  3. Joohyun Lim
  4. Elda M Munivez
  5. Marilyn Archer
  6. David M Hudson
  7. Sara F Tufa
  8. Douglas R Keene
  9. Kevin Lei
  10. Dongsu Park
  11. Cole D Kuzawa
  12. Catherine G Ambrose
  13. David R Eyre
  14. Brendan H Lee
(2021)
Tendon and motor phenotypes in the Crtap-/- mouse model of recessive osteogenesis imperfecta
eLife 10:e63488.
https://doi.org/10.7554/eLife.63488
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Abstract

Osteogenesis imperfecta (OI) is characterized by short stature, skeletal deformities, low bone mass, and motor deficits. A subset of OI patients also present with joint hypermobility; however, the role of tendon dysfunction in OI pathogenesis is largely unknown. Using the Crtap-/- mouse model of severe, recessive OI, we found that mutant Achilles and patellar tendons were thinner and weaker with increased collagen cross-links and reduced collagen fibril size at 1- and 4-months compared to wildtype. Patellar tendons from Crtap-/- mice also had altered numbers of CD146+CD200+ and CD146-CD200+ progenitor-like cells at skeletal maturity. RNA-seq analysis of Achilles and patellar tendons from 1-month Crtap-/- mice revealed dysregulation in matrix and tendon marker gene expression concomitant with predicted alterations in TGF-β, inflammatory, and metabolic signaling. At 4-months, Crtap-/- mice showed increased αSMA, MMP2, and phospho-NFκB staining in the patellar tendon consistent with excess matrix remodeling and tissue inflammation. Finally, a series of behavioral tests showed severe motor impairments and reduced grip strength in 4-month Crtap-/- mice – a phenotype that correlates with the tendon pathology.

Introduction

Tendon is a fibrous tissue that connects skeletal muscle to bone to facilitate motion, whereas ligaments connect articulating bones to support joint alignment and function (Nourissat et al., 2015; Screen et al., 2015). The extracellular matrix of tendons/ligaments is primarily composed of type I collagen as well as smaller quantities of other collagens and proteoglycans (Kannus, 2000). During development, the collagen fibrils in tendons and ligaments develop through addition and lengthening before transitioning to the appositional fusion of existing fibers with continued lengthening in postnatal life (Kalson et al., 2015). The synthesis and assembly of this collagen-rich matrix are influenced by other minor collagens and proteoglycans as well as by the cross-linking chemistry of type I procollagen fibrils, which in turn regulates fibril size and strength (Saito and Marumo, 2010). Like tendon and ligament, the organic matrix of bone consists largely of type I collagen (Alford et al., 2015), and disruptions in collagen synthesis and folding are known to negatively impact its biochemical and mechanical properties in connective tissue diseases such as Osteogenesis Imperfecta (OI) (Lim et al., 2017a). However, despite evidence of joint mobility phenotypes and motor deficits in OI patients (Arponen et al., 2014; Primorac et al., 2014), tendon and ligament phenotypes in this disease are relatively understudied.

OI is a heterogeneous group of disorders characterized by variable short stature, skeletal deformities, low bone mass, and increased bone fragility. Approximately 80% of OI cases are caused by dominantly inherited mutations in the genes encoding the α1(I) or α2(I) chains of type I collagen. Mutations in genes responsible for the synthesis, post-translational modification, and processing of collagen, such as cartilage-associated protein (CRTAP), lead to severe, recessive forms of this disease (Lim et al., 2017a). In addition to skeletal defects, other connective tissue manifestations, including joint hypermobility and skin hyperlaxity, are observed in a subset of OI patients (Arponen et al., 2014; Primorac et al., 2014). Our and others’ studies have shown that CRTAP forms a complex with Prolyl 3-hydroxylase 1 (P3h1) and Cyclophilin B (CypB, encoded by Ppib) and is required for prolyl 3-hydroxylation of type I procollagen at Pro986 of chain α1(I) and Pro707 of chain α2(I) (Hudson and Eyre, 2013; Morello et al., 2006; Baldridge et al., 2008). In this regard, loss of either CRTAP or P3H1 leads to loss of this complex and its activity, causing a severe recessive form of OI characterized by short stature and brittle bones (Morello et al., 2006; Barnes et al., 2006; Cabral et al., 2007; van Dijk et al., 2009). Collagen isolated from Crtap-/- and P3h1-/- mice is characterized by lysine over-modifications and abnormal fibril diameter (Morello et al., 2006; Cabral et al., 2007). While a comprehensive analysis of Crtap-/- mice has revealed multiple connective tissue abnormalities, including in bones, lungs, kidneys, and skin (Baldridge et al., 2010; Grafe et al., 2014), the impact of the loss of CRTAP on tendons and ligaments remains unknown.

Alterations in collagen fibril size and cross-linking have been noted in a limited number of studies using dominant or recessive mouse models of OI (Chen et al., 2014; Terajima et al., 2016; Vranka et al., 2010); however, whether loss of CRTAP impacts tendon and ligament development and structure remains unknown. In this study, we show that Crtap-/- mice have weaker and thinner Achilles and patellar tendons at 1 and 4 months-of-age that are hypercellular with a reduction in tendon volume – a phenotype absent at postnatal day 10 (P10). Examining the collagen matrix, we found an increase in stable (irreversible) collagen cross-links at both timepoints, accompanied by alterations in fibril diameter at 4-months compared to wildtype controls. RNA-seq analyses revealed both shared and distinct changes in the transcriptome of the Achilles and patellar tendons of Crtap-/- mice compared to wildtype with a predicted activation of transforming growth factor-β (TGF-β) and inflammatory signaling in both tissues. Changes in gene expression assessed by qRT-PCR revealed an upregulation of several tendon markers in Crtap-/- Achilles tendons at 1-month, including scleraxis (Scx), type I collagen α1 chain (Col1a1), lumican (Lum), tenascin-C (Tnc), and tenomodulin (Tnmd). At the same time, markers of vascularization (i.e., CD31), and collagen extracellular matrix (ECM) (i.e., type I collagen α2 chain (Col1a2), type II collagen α1 chain (Col2a1), type III collagen α1 chain (Col3a1), type IX collagen α2 chain (Col9a2)) were not different between groups. Many of these changes were also observed in our RNA-seq experiments. Consistent with the gene expression data at 1-month, 4-month-old Crtap-/- mice showed increased α smooth muscle actin (αSMA), matrix metalloproteinase-2 (MMP2), and phospho-nuclear factor kappa B (NFκB) in the patellar tendon consistent with excess matrix remodeling and tissue inflammation. These changes in Crtap-/- tendons were accompanied by motor deficits and reduced strength at 4 months-of-age. In conclusion, loss of CRTAP in mice causes abnormalities in load-bearing tendons and significant behavioral impairments.

Results

Tendon structure, size, and strength are altered in Crtap-/- mice at 1- and 4-months

Mice lacking CRTAP present with growth delay, rhizomelia, and severe osteoporosis together with disruption of other connective tissues, including lung and skin (Morello et al., 2006; Baldridge et al., 2010). To assess abnormalities in the load-bearing tendons from Crtap-/- mice, we harvested ankle and knee joints at 1 and 4 months-of-age to histologically examine the Achilles and patellar tendons. At 1-month, Crtap-/- mice presented with thinner Achilles and patellar tendons (Figure 1C,F) compared to wildtype (Figure 1A,D) and heterozygous mice (Figure 1B,E) with increased cell density in both structures (Figure 1M). By 4 months-of-age, Crtap-/- Achilles and patellar tendons remained thinner and hypercellular compared to wildtype and heterozygous mice (Figure 1G–L,N). Interestingly, ectopic chondrogenesis was present towards either end of the patellar tendon in some (but not all) 4-month-old Crtap-/- mice (Figure 1L) – a phenomenon that can occur in tendinopathy (Steinmann et al., 2020). Consistent with our histological data, phase-contrast µCT analysis demonstrated that patellar tendon volume was reduced in Crtap-/-, but not in heterozygous mice, compared to wildtype controls (Figure 1O–Q). In contrast, no significant changes in articular cartilage volume or surface were observed (Figure 1R,S).

Figure 1
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Loss of CRTAP causes thinning, hypercellularity, and weakening of tendons in young and mature mice.

(A–C) Representative H & E images of 1-month ankle joints. (D–F) Representative H & E images of 1-month knee joints. (G–I) Representative H & E images of 4-month ankle joints. (J–L) Representative H & E images of 4-month knee joints. For all micrographs, higher magnification images of the mid-tendon are illustrated. n = 3–4 mice per group. Scale bar is 1 mm. (M–N) Quantification of cell density for Achilles and patellar tendons of wildtype and Crtap-/- mice at 1 month (M) and 4 months (N) of age. Data are min-to-max box and whisker plots with individual points indicated. n = 3 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using two-tailed unpaired t-tests. Exact p-values are reported. (O–P) Representative phase-contrast μCT images of 4-month wildtype (O) and Crtap-/- (P) knee joints. Blue indicates the patellar tendon, green indicates the femoral articular cartilage, and red indicates the tibial articular cartilage. Scale bar is 1 mm. (Q) Quantification of the patellar tendon volume in wildtype, heterozygous, and Crtap-/- mice at 4-months. Data are min-to-max box and whisker plots with individual points indicated. n = 3 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using one-way ANOVA with Tukey’s post-hoc tests. Exact p-values are reported. (R–S) Quantification of articular cartilage volume (R) and surface (S) in wildtype, heterozygous, and Crtap-/- mice at 4-months. Data are min-to-max box and whisker plots with individual points indicated. n = 5 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using one-way ANOVA with Tukey’s post-hoc tests. Exact p-values are reported. (T–U) Biomechanical assessment of ultimate load (T) and linear stiffness (U) for Achilles tendons from 1-month-old wildtype, heterozygous, and Crtap-/- mice. Data are min-to-max box and whisker plots with individual points indicated. n = 3–8 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using one-way ANOVA with Tukey’s post-hoc tests. Exact p-values are reported.

To determine whether the altered structure of Crtap-/- load-bearing tendons results in reduced tissue strength, we performed biomechanical testing at 1-month on Achilles tendons to examine structural properties. As predicted based on the histological data, we observed decreases in ultimate load and linear stiffness for Crtap-/- Achilles tendons compared to heterozygous and wildtype mice (Figure 1T,U). Taken together, load-bearing tendons in Crtap-/- mice present with reduced size, increased cell density and decreased strength compared to controls.

Given Crtap is deleted throughout development in our global knockout mouse model, we next examined changes in the Achilles and patellar tendons at postnatal day 10. Interestingly, the Crtap-/- Achilles tendons (Figure 2A,B) but not the patellar tendons (Figure 2C,D) were slightly thinner (although not significant) compared to wildtype mice (Figure 2F), with no differences in cell density seen in either tissue (Figure 2E). Taken together, this data suggests that the tendon phenotypes observed at 1-month and beyond occur postnatally and are not due to defects in tendon development.

Figure 2
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Tendon thinning and hypercellularity are not observed in Crtap-/- mice at postnatal day 10.

(A–B) Representative H & E images of postnatal day 10 (P10) ankle joints. (C–D) Representative H & E images of P10 knee joints. For all micrographs, higher magnification images of the mid-tendon are illustrated. n = 5 mice per group. Scale bar is 0.5 mm. (E) Quantification of cell density and (F) Average tissue area for Achilles and patellar tendons of wildtype and Crtap-/- mice at P10 (taken mid-tendon). Data are min-to-max box and whisker plots with individual points indicated. n = 5 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using two-tailed unpaired t-tests. Exact p-values are reported.

Given the significant hypercellularity seen in the load-bearing tendons from Crtap-/- mice, we next examined whether there were changes in tenocyte populations associated with progenitors and tendon repair response in Crtap-/- mice. Specifically, previous literature has demonstrated that progenitor-like cells involved in tendon maturation and repair are marked by the expression of CD146 (Lee et al., 2015) in addition to others. Using fluorescence-activated cell sorting (FACS) analysis of 5-month-old patellar tendons, we observed a significant decrease in the percentage of CD45-CD31-CD146+CD200+ (~2%) compared to wildtype mice (~4%) (Figure 3A–C, red box). In contrast, CD45-CD31-CD146-CD200+ cells were concomitantly increased in Crtap-/- mice (Figure 3D). Taken together, this data suggests that the matrix disruptions caused by loss of CRTAP may lead to the dysregulation of discrete tendon cell populations within the adult patellar tendon.

Figure 3
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Loss of CRTAP in the patellar tendon leads to a decrease in progenitor cells and an accumulation of immature resident tissue cells.

(A–B) Patellar tendon cells isolated from 5-month-old wildtype (A) or Crtap-/- (B) mice were analyzed for the expression of CD200 and CD146 tendon progenitor markers (top histogram) within the CD45-CD31- population (bottom histogram). The plots are representative from a single wildtype or Crtap-/- mouse. (C–D) Graphs show the percentage of CD45-CD31-CD146+CD200+ progenitor cells (C) and CD45-CD31-CD146-CD200+ immature tendon cells (D) From 5-month wildtype and Crtap-/- patellar tendons. Data are min-to-max box and whisker plots with individual points indicated. n = 5 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using two-tailed unpaired t-tests. Exact p-values are reported.

Collagen fibril formation is altered in heterozygous and Crtap-/- mice

Tendons develop embryonically by increasing in fibril length and number, whereas postnatal growth arises from an increase in fibril length and diameter – the latter of which is driven by the lateral fusion of smaller fibrils (Kalson et al., 2015). To investigate the role of CRTAP in postnatal collagen fibril maturation, we utilized transmission electron microscopy (TEM) to examine changes in fibril diameter in flexor digitorum longus (FDL), Achilles, and patellar tendons (Figure 4). In the FDL tendon, there was a marked increase in small collagen fibrils (20–60 nm in size), a reduction in 80–320 nm fibrils, and a slight increase in larger fibrils (>340 nm in diameter) in Crtap-/- mice compared to wildtype (Figure 4A,C,J). Despite similarities seen in histology, heterozygous mutant FDL tendons also exhibited a slight increase in 20–40 nm fibrils in mice compared to wildtype controls (Figure 4A–B,J). Similar trends were observed for the Achilles tendon, namely an increase in small fibrils (20–60 nm), a reduction in 80–240 nm fibrils, and an increase in large fibrils (>280 nm) upon loss of Crtap (Figure 4D,F,K). In contrast to what we observed for the FDL, heterozygous Achilles tendons did not have increased numbers of smaller fibers (Figure 4E,K). Instead, a greater number of fibrils ranging from 140-to-200 nm in size were noted compared to wildtype controls.

Figure 4
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Collagen fibril diameter is altered in tendons from heterozygous and Crtap-/- mice.

(A–C) Representative transverse TEM images of 4-month (A–C) FDL tendon collagen fibrils, (D–F) Achilles tendon collagen fibrils, and (G–I) patellar tendon collagen fibrils. Scale bar is 500 nm. (J) Representative histogram of the size distribution for collagen fibrils in FDL tendons. Data are representative of n = 3 mice. (K) Representative histogram of the size distribution for collagen fibrils in Achilles tendons. Data are representative of n = 3 mice. (L) Representative histogram of the size distribution for collagen fibrils in patellar tendons. Data are representative of n = 3 mice per group. (M–R) Representative longitudinal TEM images of 4-month wildtype FDL (M), Achilles (N), and patellar (O) tendons, and 4-month Crtap-/- FDL (P), Achilles (Q), and patellar (R) tendons. Scale bar is 500 nm.

Compared to the FDL and Achilles tendons, the most significant differences were seen within the patellar tendon, although the pattern of changes remained consistent (Figure 4G–I,L). Specifically, we observed a dramatic increase in 20 nm collagen fibrils compared to heterozygous and wildtype mice (Figure 4G–I,L). Fibrils ranging from 100-to-180 nm in diameter were reduced in heterozygous and Crtap-/- mice compared to wildtype. Interestingly, the greatest difference from wildtype was an increase in large collagen fibrils (>200 nm) in both heterozygous and Crtap-/- mice (Figure 4G–I,L).

To examine how collagen fibril alignment is affected by the loss of CRTAP, we examined longitudinal sections of FDL, Achilles, and patellar tendons from 4-month wildtype and Crtap-/- mice using TEM (Figure 4M–R). Consistent with our transverse data, we observed a wider array of thinner and thicker collagen fibrils in Crtap-/- tendons (Figure 4P,Q,R) compared to wildtype (Figure 4M,N,O). In addition, while the collagen fibrils in wildtype animals were well-aligned, collagen fibril alignment in Crtap-/- tendons was more irregular (Figure 4P,Q,R). Taken together, these data indicate that loss of CRTAP alters collagen fibril assembly and alignment in load-bearing tendons. In addition, the degree to which collagen assembly is affected is site-dependent.

Collagen cross-linking is increased in heterozygous and Crtap-/- mice

Along with P3H1 and CyPB, CRTAP is an integral part of the collagen prolyl 3-hydroxylation complex responsible for the 3-hydroxylation of Pro986 of the type I procollagen α1 chain (Lim et al., 2017a). Loss of this complex blocks 3-hydroxyproline formation and affects lysine hydroxylation and cross-linking in bone collagen (Morello et al., 2006; Baldridge et al., 2008); however, whether Crtap-/- tendons display altered collagen cross-linking is unknown. To investigate this, we harvested tendons at 1- and 4-months and assessed collagen cross-linking by quantifying the levels of hydroxylysyl-pyridinoline (HP) (Figure 5). Overall, we observed an increase in these stable, mature collagen cross-links from 1 to 4 months-of-age in all genotypes for the FDL and Achilles tendons (Figure 5A–B). In contrast, for the patellar tendon, age-dependent increases in collagen cross-links were only observed in Crtap-/- mice (Figure 5C). For FDL tendons, Crtap-/- mice had more of these collagen cross-links at 1- and 4-months compared to heterozygous and wildtype mice; however, the content of HP residues per collagen decreased with age in this tissue (Figure 5A). Interestingly, in Achilles tendons, an increase in collagen cross-linking was observed in both heterozygous and Crtap-/- mice at 1-month compared to wildtype. In contrast, at 4-months, only Crtap-/- mice had elevated collagen cross-links, and these levels were greater than those observed at the earlier time point (Figure 5B).

Figure 5
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Collagen cross-linking is increased in tendons from young and mature Crtap-/- mice.

Quantification of collagen cross-links as hydroxylysyl-pyridinoline (HP) residues per collagen molecule for (A) FDL tendons; (B) Achilles tendons; and (C) patellar tendons. Data are shown as means ± S.D. n = 3–4 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using one-way ANOVA with Tukey’s post-hoc tests. Exact p-values are reported.

The patellar tendon showed the greatest increase in collagen cross-links both with time and across genotypes of the tissues examined. Specifically, collagen cross-links were elevated by 5- to 10-fold in Crtap-/- patellar tendons compared to heterozygous and wildtype at 1- and 4-months, respectively (Figure 5C). Taken together, these data suggest that CRTAP is required for proper hydroxylation and cross-linking of collagen fibrils in tendons in a semi-dominant fashion, as heterozygous mutant tendons display a phenotype that is milder than the phenotype observed for homozygous mutant mice. Notably, the chemical quality of collagen cross-linking appears to be spatiotemporally regulated, and this regulation is differentially affected by the loss of a single or both copies of Crtap.

Signaling and metabolic dysregulation in Crtap-/- load-bearing tendons

We performed bulk RNA-seq with RNA isolated from Achilles and patellar tendons of 1-month-old wildtype and Crtap-/- mice to investigate the molecular changes underlying the observed tendon phenotypes. To determine global changes in differentially expressed genes and predicted upstream regulators, we performed Ingenuity Pathway Analysis (IPA, Qiagen, Germany). For the Achilles tendon, a total of 178 genes (consisting of 99 upregulated genes and 79 downregulated genes) were significantly differentially expressed between wildtype and Crtap-/- samples (Figure 6A). Of the top 30 differentially expressed genes, several ECM proteins, including matrilin-3 (Matn3), matrilin-4 (Matn4), and fibronectin 1 (Fn1), and proteolytic enzymes such as matrix metallopeptidas-2 (Mmp2) were dysregulated. Gene ontology analysis revealed ‘GO:000715 – Cell Adhesion’, ‘GO:0045778 – Positive Regulation of Ossification’, and ‘GO:0051928 – Positive Regulation of Calcium Ion Transport’ to be enriched (Figure 6B). Examination of upstream regulators based on the differential gene expression data revealed a predicted activation of TGF-β1 in Crtap-/- mice and predicted inhibition of dystrophin (DMD) along with several for which activation state was unclear, including platelet-derived growth factor-BB (PDGF-BB), β-catenin (CTNNB1), and tumor necrosis factor (TNF) (Figure 6C).

Figure 6
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Transcriptome analysis of tendons from 1-month-old Crtap-/- mice.

DESeq2 was used to compare gene expression between wildtype and Crtap-/- Achilles and patellar tendon RNA samples, and genes with an adjusted p-value<0.05 and absolute log2 fold change >1 were considered as differentially expressed. (A) A bi-clustering heatmap of the top 30 differentially expressed genes between wildtype and Crtap-/- Achilles tendons sorted by adjusted p-value and plotted according to log2 transformed expression values. The Wald test was used to generate p-values and log2 fold changes. See Figure 6—source data 1 for a complete list of differentially regulated genes. (B) Significantly differentially expressed genes between Achilles tendons from wildtype and Crtap-/- mice were clustered by their gene ontology, and enrichment for gene ontology terms was tested using Fisher exact test. All gene ontology terms with an adjusted p-value<0.05 are plotted according to their -log10 adjusted p-value. (C) Select upstream regulators predicted as being activated (shown in green), inhibited (shown in red), or of unclear state (shown in gray) in Crtap-/- compared to wildtype Achilles tendons plotted according to their -log10 adjusted p-value. See Figure 6—source data 2 for a complete list of predicted upstream regulators. n = 3 mice per genotype for (A–C). (D) A bi-clustering heatmap of the top 30 differentially expressed genes between wildtype and Crtap-/- patellar tendons sorted by adjusted p-value and plotted according to log2 transformed expression values. The Wald test was used to generate p-values and log2 fold changes. See Figure 6—source data 3 for a complete list of differentially regulated genes. (E) Significantly differentially expressed genes between patellar tendons from wildtype and Crtap-/- mice were clustered by their gene ontology, and enrichment for gene ontology terms was tested using Fisher exact test. All gene ontology terms with an adjusted p-value<0.05 are plotted according to their -log10 adjusted p-value. (F) Select upstream regulators predicted as being activated (shown in green), inhibited (shown in red), or of unclear state (shown in gray) in Crtap-/- compared to wildtype patellar tendons plotted according to -log10 adjusted p-value. See Figure 6—source data 4 for a complete list of predicted upstream regulators. n = 2 mice per genotype for (D–F).

Figure 6—source data 1

List of differentially expressed genes between 1-month wildtype and Crtap knockout Achilles tendons.

The Wald test was used to generate p-values and log2 fold changes. Genes with an adjusted p-value<0.05 and absolute log2 fold change >1 were called significantly differentially expressed genes. This is a full list of all differentially expressed genes ordered by adjusted p-value.

https://cdn.elifesciences.org/articles/63488/elife-63488-fig6-data1-v2.xlsx
Figure 6—source data 2

Predicted upstream regulators driving differential gene expression between 1-month wildtype and Crtap knockout Achilles tendons.

Based on a list of differentially expressed genes, upstream regulators were predicted using Ingenuity Pathway Analysis. The results are sorted by adjusted p-value.

https://cdn.elifesciences.org/articles/63488/elife-63488-fig6-data2-v2.xlsx
Figure 6—source data 3

List of differentially expressed genes between 1-month wildtype and Crtap knockout patellar tendons.

The Wald test was used to generate p-values and log2 fold changes. Genes with an adjusted p-value<0.05 and absolute log2 fold change >1 were called significantly differentially expressed genes. This is a full list of all differentially expressed genes ordered by adjusted p-value.

https://cdn.elifesciences.org/articles/63488/elife-63488-fig6-data3-v2.xlsx
Figure 6—source data 4

Predicted upstream regulators driving differential gene expression between 1-month wildtype and Crtap knockout patellar tendons.

Based on a list of differentially expressed genes, upstream regulators were predicted using Ingenuity Pathway Analysis. The results are sorted by adjusted p-value.

https://cdn.elifesciences.org/articles/63488/elife-63488-fig6-data4-v2.xlsx

In keeping with the increased phenotypic severity seen in patellar tendons from Crtap-/- mice, a greater number of total genes were differentially expressed between wildtype and Crtap-/- patellar tendons (Figure 6D). We saw significant differential expression of 519 genes, with 224 being upregulated and 295 downregulated in Crtap-/- compared to wildtype. Several of the top 30 differentially expressed genes were minor collagens such as type IX collagen α3 chain (Col9a3), type IX collagen α1 chain (Col9a1), and type XXII collagen α1 chain (Col22a1), as well as other ECM proteins, including lumican (Lum) and fibronectin 1 (Fn1). Unlike the Achilles tendon, gene ontology analysis revealed significant enrichment for metabolic processes, including ‘GO:0055114 – Oxidation-Reduction Process’, ‘GO:0050873 – Brown Fat Cell Differentiation’, and ‘GO:0050872 – White Fat Cell Differentiation’ as well as for ‘GO:0008284 – Positive Regulation of Proliferation’ and ‘GO:0001525 – Angiogenesis’ (Figure 6E). Examination of upstream regulators also suggested a highly significant activation of TNF and interleukin 6 (IL-6) as well as fibroblast growth factor 2 (FGF2) and TGF-β3 in Crtap-/- patellar tendons (Figure 6F). Indeed, the representation of TNF, TGF-β, and PDGF-BB in this dataset is consistent with but more severe than that observed for those same regulators in the Achilles tendon results (Figure 6C).

We next examined the expression patterns of genes that are implicated in postnatal tendon maturation and homeostasis. We confirmed the loss of Crtap expression in Crtap-/- Achilles tendon compared to wildtype – a finding also demonstrated in our RNA-seq data (RNA-seq data shown in red as ‘log2 fold change; adjusted p-value’ with the graphed qPCR results in Figure 7). Interestingly, loss of CRTAP led to a modest upregulation in Scx expression with no changes in Mkx and Egr1 transcript levels (Figure 7). Despite a modest downregulation in Col1a1 transcripts in Crtap-/- Achilles tendons, there were no changes in the expression of Col1a2, Col2a1, Col3a1, or Col9a2. On the other hand, we observed an increase in expression of several ECM glycoproteins and small leucine-rich proteoglycans (SLRPs), including Tnc, Lum, Tnmd, and Fn1, known to be upregulated during tendon maturation and repair. We also observed an upregulation in Thbs3 transcripts in Crtap-/- Achilles tendons compared to wildtype, consistent with our RNA-seq data (Figure 7). Overall, we speculate that the modest reduction in Col1a1 expression and altered expression of Scx, as well as other ECM proteins such as Tnc, Lum, and Tnmd, could be associated with the observed aberrations in collagen fibrillogenesis seen in Crtap-/- mice, and may indicate an increased remodeling or repair response similar to that seen in OI bone (Grafe et al., 2014).

Figure 7
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Tendon marker gene expression is altered in Crtap-/- Achilles tendons at 1 month.

Real-time quantitative PCR was performed to examine changes in the expression of Crtap, various fibrillar collagens (i.e., Col1a1, Col1a2, Col2a1, Col3a1, Col9a2), tendon makers (i.e. Scx, Mkx, Egr1, Tnc, Lum, Tnmd, Fn1, Fbn1), other targets from the RNA-seq analysis in Figure 6 (i.e., Thbs3), and CD31 as a marker of vascularization. n = 4 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using one-way ANOVA with Tukey’s post-hoc tests. Exact p-values are reported. The log2 fold change and adjusted p-value (shown as log2 fold change; adjusted p-value") from the RNA-seq experiment in Figure 6 is indicated in red just below the gene name.

To investigate whether loss of CRTAP was associated with increased ECM remodeling at skeletal maturity, we performed a series of immunohistochemistry experiments at 4 months-of-age (Figure 8). Interestingly, Herovici staining revealed an abundance of immature collagen in patellar tendons from Crtap-/- mice compared to wildtype, as evidenced by the prominent blue staining (Figure 8A,B). We also observed increased α smooth muscle actin (αSMA; Figure 8C,D) and MMP2 (Figure 8E,F) together with elevated levels of phosphorylated nuclear factor kappa B (NFκB; Figure 8G,H), consistent with our RNA-seq data and our hypothesis that Crtap-/- tendons exist in a state of increased remodeling/repair and inflammation.

Figure 8
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Four-month Crtap-/- patellar tendons exhibit increased staining for markers of fibrosis, increased ECM turnover, and inflammatory events.

(A–B) Representative herovici-stained images of 4-month patellar tendons. (C–D) Representative αSMA IHC images of 4-month patellar tendons. (E–F) Representative MMP2 IHC images of 4-month patellar tendons. (G–H) Representative phosphorylated NFκB (pNFκB) IHC images of 4-month patellar tendons. For all micrographs, higher magnification images of the mid-tendon are illustrated. n = 3–5 mice per group. Scale bar is 0.5 mm.

Loss of CRTAP leads to deficiencies in motor activity, coordination, and strength

Based on the observed defects in Crtap-/- tendons, we performed a series of behavioral assays at 4 months-of-age to assess motor phenotypes. Using the open-field assay to quantify changes in spontaneous motor activity, we observed that Crtap-/- mice displayed significant reductions in both horizontal and vertical activity compared to heterozygous and wildtype mice (Figure 9A–B). We next examined changes in motor coordination and endurance using the rotarod assay. While no genotype-dependent differences were observed during the learning phase of the assessment (Trials 1–5), Crtap-/- displayed a reduction in latency to fall for Trials 6, 9–10 compared to wildtype and Trials 6, 8–10 compared to heterozygous mice (Figure 9C). To confirm this observation, we evaluated the mice using the grid foot slip assay – an alternative metric for motor coordination. In this regard, we found that Crtap-/- mice exhibited a modest increase in forelimb and hindlimb foot slips compared to heterozygous and wildtype mice (Figure 9D–E). Taken together, these findings indicate that Crtap-/- mice have deficiencies in motor activity and coordination compared to controls.

Figure 9
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Motor activity and coordination are impaired in 4-month-old Crtap-/- mice.

(A–B) Quantification of spontaneous motor activity including horizontal (A) and vertical (B) activity over a 30-min period using the open-field assay. Data are min-to-max box and whisker plots with individual points indicated. n = 9–12 mice per group. For (A), data passed the Shapiro-Wilk test for normality, and groups were compared using one-way ANOVA with Tukey’s post-hoc tests. For (B), data failed the Shapiro-Wilk test for normality, and groups were compared using Kruskal-Wallis with Dunn’s post-hoc tests. Exact p-values are reported for (A–B). (C) Quantification of motor activity, coordination, and endurance across 10 trials conducted over 2 days using an accelerating rotarod assay. Data are means ± S.D. n = 9–12 mice per group. Groups were compared using repeated-measures two-way ANOVA with Tukey’s post-hoc tests. Exact p-values are reported, with black p-values being compared to wildtype, and blue p-values being compared to heterozygous mice. (D–E) Quantification of forelimb (D) and hindlimb (E) motor coordination using the grid foot slip assay. Data are min-to-max box and whisker plots with individual points indicated. n = 9–12 mice per group. Data failed the Shapiro-Wilk test for normality, and groups were compared using Kruskal-Wallis with Dunn’s post-hoc tests. Exact p-values are reported. (F) Quantification of forelimb and hindlimb grip strength using the inverted grid assay conducted for 120 s. A reduction in latency to fall indicates reduced strength. Data are min-to-max box and whisker plots with individual points indicated. n = 8–9 mice per group. Data failed the Shapiro-Wilk test for normality, and groups were compared using Kruskal-Wallis with Dunn’s post-hoc tests. Exact p-values are reported. (G) Quantification of forelimb grip strength in N of force measured over three trials and then averaged. Data are min-to-max box and whisker plots with individual points indicated. n = 9–12 mice per group. Data passed the Shapiro-Wilk test for normality, and groups were compared using one-way ANOVA with Tukey’s post-hoc tests. Exact p-values are reported.

We next evaluated strength in the Crtap-/- mice using the inverted grid and grip strength assays. Interestingly, we observed a decrease in the latency to fall during the inverted grid assay for Crtap-/- mice compared to heterozygous and wildtype controls (Figure 9F). Using a more quantitative metric, we examined these mice using the grip strength test and found that while wildtype and heterozygous mice could generate approximately 1.3 N of force, mice lacking CRTAP were weaker with a mean grip strength of 0.62 N (Figure 9G). Thus, Crtap-/- mice display significant reductions in strength together with perturbations in motor activity and coordination – behavioral changes that could be related in part to their tendon phenotype.

Discussion

In this study, we examined the histological, ultrastructural, biochemical, and transcriptional characteristics of load-bearing tendons in the Crtap-/- mouse model of severe, recessive OI. We demonstrate that at 1 and 4 months-of-age, Crtap-/- have thinner, more cellular Achilles and patellar tendons with a reduction in the CD146+CD200+ cell pool compared to heterozygous and wild-type mice. Importantly, we did observe only slight thinning with no increased cell density in Achilles or patellar tendons from Crtap-/- mice at P10, suggesting that the phenotype is mostly restricted to deficits in tendon maturation but not development. Examining collagen fibril organization, we found a marked alteration in collagen fibril alignment and the number of small and large fibrils in Crtap-/- mice compared to wildtype that varied in severity depending on the tendon being examined. Consistent with our TEM findings, we found that 1-month Achilles tendons from Crtap-/- mice exhibited reduced ultimate load and linear stiffness compared to wildtype; however, the reduced structural properties could also be due to a reduction in cross-sectional area of the tendon at this age. Stable, HP cross-links were also elevated at 1- and 4-months in Crtap-/- mice compared to wildtype, which indicates an increase in telopeptide lysine hydroxylation and irreversible intermolecular cross-links (see below). RNA-seq analysis revealed alterations in extracellular matrix proteins, growth factor signaling, and metabolic pathways in Crtap-/- tendons compared to wildtype controls confirmed by qRT-PCR and IHC. Finally, we demonstrate that Crtap-/- mice exhibit motor impairments concomitant with reductions in grip strength – a phenomenon that may be related to the tendon pathology and possible deficits in other musculoskeletal tissues such as muscle.

Collagen ultrastructure and cross-linking have been well-documented in the bones of mouse models for both dominant and recessive OI; however, quantitative and histological characterization of tendons in these models has been less studied. In this regard, we demonstrate that Crtap-/- mice have thinner and weaker Achilles and patellar tendons at 1- and 4-months. Despite the reduction in size and extracellular matrix, tendons from these mice are hypercellular compared to wildtype and heterozygous animals – a phenotype observed in other tissues from Crtap-/- mice, including bone, lungs, and the glomerular compartment of the kidney (Baldridge et al., 2010; Grafe et al., 2014). Indeed, defects in ECM proteins such as type I collagen are correlated with changes in the proliferation and survival of surrounding cells (Hynes, 2009). Interestingly, the pathological changes observed in load-bearing tendons from Crtap-/- mice were accompanied by a significant reduction in CD146+CD200+ cells. Given that CD146 has been implicated as a marker for tendon progenitor-like cells (Lee et al., 2015), we speculate that the decrease in CD146 at 5-months may indicate that Crtap-/- tendons are in a state of chronic remodeling/repair (see below). While the alterations in tendon size and cellularity may result from alterations in the collagen extracellular matrix, it could also be associated with alterations in cellular signaling. In this regard, TGF-β signaling is upregulated in bones from Crtap-/- mice (Grafe et al., 2014), and elevated TGF-β signaling has been noted in mouse models with increased tendon cellularity and alterations in collagen fibril distribution (Lim et al., 2017b). Indeed, our RNA-seq analysis identified TGF-β signaling as an activated upstream regulator of the differential gene expression observed in the tendons from Crtap-/- mice. We also observed significant metabolic dysregulation in Crtap-/- tendons. Interestingly, mammalian target of rapamycin complex 1 (mTORC1) knockout mouse tendons have a similar histological phenotype to those of Crtap-/- mice (Lim et al., 2017b). These data are consistent with the principle that an altered ECM can alter cellular signaling, as previously shown for vascular tissue in Marfan syndrome and OI bone.

In addition to type I collagen, other minor collagens together with glycoproteins and SLRPs are present within tendons and regulate type I collagen self-assembly and are expressed most highly during development and repair. In the present study, we demonstrated that Crtap is expressed in load-bearing tendons and that its expression is completely ablated in tendons from Crtap-/- mice. Other than a modest reduction in Col1a1, there was no significant difference in the expression of Col3a1, which is typically increased in the early stages of tendon injury and healing (Howell et al., 2017; Juneja et al., 2013; Yang et al., 2013). While Col2a1 and Col9a2 expression were upregulated in our RNA-seq data from Crtap-/- Achilles tendon, no differences were observed by qRT-PCR. Despite a lack of changes in the expression of many fibrillar collagens, we observed upregulation in the expression of Scx and various glycoproteins and SLRPs, including Tnc, Lum, Tnmd, Fn1, and Thbs3, in Crtap-/- mice. Many of these markers are upregulated during tendon injury and healing (Yang et al., 2013; Snedeker and Foolen, 2017), with Tnmd being a positive regulator of tenocyte proliferation (Docheva et al., 2005), elevated Fn1 being a precursor for tendon ECM deposition (Kadler et al., 2008), and Tnc expression being elevated under conditions of increased mechanical load (Chiquet et al., 2003; Chiquet-Ehrismann and Tucker, 2004). Taken together, this would suggest that load-bearing Crtap-/- tendons are immature and stuck in a process of perpetual remodeling and repair compared to wildtype controls, reminiscent of the increased remodeling observed in Crtap-/- bones.

In the present study, we found an increased proportion of small and large collagen fibrils in the FDL, Achilles, and patellar tendons of Crtap-/- mice. These distributions varied in severity across the three tissues, with the most significant differences observed in the patellar tendon. P3h1-/- mice have been reported to display an increased proportion of small collagen fibrils in tail tendons (Vranka et al., 2010), indicating that loss of the 3-prolyl hydroxylase complex alters collagen fibrillogenesis. At the same time, the increased number of small fibers was more pronounced in tail tendons from P3h1-/- mice, and there was no evidence of an increased proportion of large fibers (Vranka et al., 2010) as observed for Crtap-/- mice in this study. Like the P3h1-/- mouse model, mice lacking CypB also exhibit a pronounced increase in the number of small collagen fibrils within tail tendons (Terajima et al., 2016). Together, this may indicate that despite forming a complex with P3h1 and CypB, loss of Crtap has distinct consequences on collagen fibrillogenesis. At the same time, it is important to note that tail tendons were used for collagen fibril distribution assessments in both P3h1-/- and Ppib-/- mice (Terajima et al., 2016; Vranka et al., 2010), whereas load-bearing tendons were examined in our study. The difference in tissue type examined might also explain why we observed unique alterations in collagen fibril distribution in both heterozygous and Crtap-/- mice. While the focus of the present study was on load-bearing tendon phenotypes and how these may relate to joint laxity and motor deficits seen in OI patients, future work examining positional tendons of the tail could also be insightful.

Type I procollagen molecules undergo post-translational modifications within the endoplasmic reticulum, including lysyl-hydroxylation and prolyl-hydroxylation, that are critical for proper collagen synthesis, transport, and stability. Specifically, telopeptide lysine hydroxylation results in mature lysyl-pyridinoline (LP) or hydroxylysyl-pyridinoline (HP) residues after lysyl oxidase oxidation, which as permanent, irreversible crosslinks play a role in regulating fibril growth and strength (Eyre, 1987; Bateman et al., 2009). Previous literature has demonstrated that loss of the 3-prolyl hydroxylase complex caused by loss of P3H1 (P3h1-/-) or CRTAP (Crtap-/-) prevents prolyl 3-hydroxylation of clade A (type I, II, and III) collagens and can lead to changes in lysine post-translational modifications due to loss of its chaperone function (Hudson and Eyre, 2013; Morello et al., 2006). In this study, we found that mature collagen cross-links (HP residues per collagen) are markedly increased in the FDL, Achilles, and patellar tendons of Crtap-/- mice relative to wildtype. This contrasts that seen in bones from Crtap-/- mice, where there is no change in HP residues per collagen compared to wildtype. Instead, an increase in the ratio of LP/HP is observed along with a complete lack of 3-hydroxylation of Pro 986 in the chains of type I collagen (Baldridge et al., 2010; Grafe et al., 2014). Interestingly, we observed increased cross-links in the Achilles, but not FDL or patellar tendons of 1-month-old heterozygous mice, indicating a mild haploinsufficient effect of CRTAP on this tendon biochemical property, thereby suggesting a rate-limited contribution of this complex in this function. Outside of the genotype-specific effects, we saw an age-dependent increase in HP residues per collagen in all genotypes. This observation is consistent with a study by Taga and colleagues that reported an increase in 3-hydroxyproline residues in rat tendon collagen (but not bone or skin) that plateaued at 3 months-of-age (Taga et al., 2016). Together with the TEM analyses, these data suggest that altered collagen cross-linking in tendons from Crtap-/- mice may adversely affect collagen fibril assembly.

In addition to skeletal deformities and frequent fractures, severe OI is associated with motor impairments, including gait abnormalities, chronic pain, and reduced muscle strength (Arponen et al., 2014; Primorac et al., 2014; Garman et al., 2019). In this study, we showed that Crtap-/- mice exhibit reduced horizontal and vertical motor activity using the open field assay and reduced motor coordination and endurance using the rotarod and grid foot slip assays. We also observed a reduction in latency to fall on the inverted grid assay mirrored by a dramatic loss of grip strength compared to heterozygous and wildtype mice. These results are consistent with findings reported for the Col1a1Jrt/+ mouse model of severe OI and Ehlers-Danlos syndrome (Chen et al., 2014). Specifically, Abdelaziz and colleagues found that Col1a1Jrt/+ mice displayed reduced motor activity using the open field and running wheel assays – a phenotype they attributed to thermal hyperalgesia and mechanical allodynia in these mice (Abdelaziz et al., 2015). While the reduced vertical activity may indicate a pain or spinal phenotype, changes in motor coordination and grip strength in Crtap-/- mice are likely more related to deficits in the muscle-tendon unit. Indeed, muscle dysfunction has been noted in OI patients and various preclinical mouse models (Berman et al., 2020; Gremminger et al., 2019; Veilleux et al., 2017). Unfortunately, given only a global Crtap knockout mouse line was used here, understanding the contribution of muscle independent of the tendon is complex and needs further study. Despite these limitations, our study describes the most comprehensive characterization of motor and strength deficits in a mouse model of severe, recessive OI to date, providing a useful set of functional outputs with which to evaluate future therapeutics or to interrogate the role of tendon and other musculoskeletal tissues in motor function.

Taken together, this study provides the first evidence for load-bearing tendon phenotypes in the Crtap-/- mouse model of severe, recessive OI. We also provide compelling evidence for a strong motor activity and coordination phenotype in these mice. As the quality of life is so impacted in patients with OI, a more comprehensive evaluation of behavioral outcomes in future preclinical studies may provide important insights into the efficacy of therapeutic interventions.

Materials and methods

Key resources table
Reagent type (species) or resourceDesignationSource or referenceIdentifiersAdditional information
Genetic reagent (M. musculus)Crtaptm1BrleB. H. Lee LaboratoryDOI: 10.1016/j.cell.2006.08.039Deposited at Jackson Labs (B6; 129S7-Crtaptm1Brle/J; Stock #: 018831)
Genetic reagent (M. musculus)129sv/EVDr. Allan BradleyBaylor College of MedicineMaintained in Lee Laboratory for many generations
Genetic reagent (M. musculus)C57BL/6JJackson LaboratoryStock #: 000664
RRID:IMSR_JAX:000664
AntibodyAnti-CD45- pacific blue (mouse monoclonal)InvitrogenCat. #: MCD4528
RRID:AB_10373710		FACS (1:100)
Clone: 30-F11
AntibodyAnti-CD31-eFluor 450 (mouse monoclonal)InvitrogenCat. #: 48-0311-82
RRID:AB_10598807		FACS (1:100)
Clone: 390
AntibodyAnti-CD146-PE-Cy7 (mouse monoclonal)BioLegendCat. #: 134713
RRID:AB_2563108		FACS (1:100)
Clone: ME-9F1
AntibodyAnti-CD200-APC (mouse monoclonal)BioLegendCat. #: 123809
RRID:AB_10900996		FACS (1:100)
Clone: OX-90
AntibodyAnti-αSMA (rabbit polyclonal)AbcamCat #: ab5694
RRID:AB_2223021		IHC (1:200)
AntibodyAnti-MMP2 (goal polyclonal)R and D SystemsCat #: AF1488
RRID:AB_2145989		IHC (1:400)
AntibodyAnti-phospho-NFκB p65 (Ser536) (93H1) (rabbit monoclonal)Cell SignalingCat #: 3033
RRID:AB_331284		IHC (1:20)
AntibodyBiotin-SP-AffiniPure Donkey Anti-Rabbit IgG (H + L)Jackson ImmunoResearch LabsCat #: 711-065-152
RRID:AB_2340593		IHC (1:100, 1:400)
AntibodyBiotin-SP-AffiniPure Donkey Anti-Goat IgG (H + L)Jackson ImmunoResearch LabsCat #: 705-065-147
RRID:AB_2340397		IHC (1:500)
AntibodyPeroxidase-Streptavidin
Slides were incubated with DAB substrate (Vector Laboratories, SK-4100)		Jackson ImmunoResearch LabsCat #: 016-030-084
RRID:AB_2337238		IHC (1:100, 1:400, 1:500)
AntibodyDAB Substrate Kit (3,3’-diaminobenzidine)Vector LaboratoriesCat #: SK-4100
RRID:AB_2336382
OtherPropidium iodideSigma-AldrichCat. #: P4170-100MG
Commercial assay or kitRNeasy fibrous tissue mini kitQiagenCat. #: 74704
Commercial assay or kitRNeasy micro kitQiagenCat. #: 74004
Commercial assay or kitiScript cDNA synthesis kitBio-RadCat. #: 1708890
Chemical compound, drugLightCycler FastStart DNA Master SYBR Green IRocheCat. #: 12239264001
Chemical compound, drugHexaammineruthenium(III) chlorideSigma-AldrichCat. #: 262005–5G0.7% w/v in phase-contrast µCT fixative, wash buffer, and post-fixative
Chemical compound, drugGlutaraldehydePolysciences, IncCat. #: 019092% v/v in phase-contrast µCT fixative
Chemical compound, drugCacodylic acidElectron Microscopy SciencesCat. #: 122000.05 M in phase-contrast µCT fixative and wash buffer; 0.1 M for post-fixative
Chemical compound, drugOsmium tetroxideElectron Microscopy SciencesCat. #: 191901% w/v in phase-contrast µCT or TEM post-fixative
Software, algorithmFijiImageJhttps://imagej.net/Fiji
RRID:SCR_002285		Version 2.1.0/1.53 c
Software, algorithmGraphPad PrismGraphPad Softwarehttps://graphpad.com
RRID:SCR_002798		Version 9.0.1
Software, algorithmTri/3D BONRatoc System Engineeringhttps://www.ratoc.co.jp/ENG/3diryo.htmlVersion R.8.00.008-H-64
Software, algorithmFlowJoBDhttps://www.flowjo.com/solutions/flowjo/downloads
RRID:SCR_008520		Version 10.7

Animals

Crtap−/− mice were generated as previously described (Morello et al., 2006) and maintained on a mixed C57BL/6J and 129Sv genetic background. Male mice were used for all experiments. All studies were performed with approval from the Institutional Animal Care and Use Committee (IACUC) at Baylor College of Medicine. Mice were housed three to four mice to a cage in a pathogen-free environment with ad libitum access to food and water and under a 14 hr light/10 hr dark cycle.

Histological analysis

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Mice were euthanized and ankle and knee joints were dissected and fixed for 48 hr on a shaker at 4°C or room temperature in freshly prepared 4% paraformaldehyde (PFA) in 1 × phosphate buffered saline (PBS). Samples were decalcified at 4°C using 10% ethylenediaminetetraacetic acid (EDTA) in 1 × PBS for 10 days (with one change out at 5 days) before paraffin embedding using a standard protocol. Samples were sectioned at 6 μm and stained with hematoxylin and eosin (H and E) to visualize tendon structures. Herovici staining was performed on separate sections to visualize the ratio of mature collagen (red color) to more immature collagen and reticular fibers (blue color). Using H and E-stained tissue sections, cell number per tissue area as well as tissue area were determined using the Fiji release of ImageJ (Schindelin et al., 2012). For the 1-month and 4-month time points, two to threeregions of interest were selected in one plane-matched tissue section for each animal and used for quantification. For postnatal day 10 (P10), a single region of interest was selected across three different sections for each animal owing to the smaller size of the tissue at this earlier time point. For cell density, the number of cells was then divided by the tissue area to determine cell density.

Fluorescence-activated cell sorting analysis of tendon progenitors

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After dissection of patellar tendons from 5-month-old wildtype and Crtap-/- mice, tissues were cut into small pieces in 1 × PBS with 10% fetal bovine serum (FBS) and incubated with 500 µl of PBS + 10% FBS and 0.1% collagenase at 37°C for 3 hr. After digestion, cells were filtered with a 40 μm strainer, washed, resuspended in 1 × PBS at a concentration of 106 cells/mL, and stained with CD45-pacific blue (clone: 30-F11), CD31-eFlour 450 (clone: 390), CD146-PE-Cy7 (clone ME-9F1) and CD200-APC (clone OX-90) (eBioscience). Propidium iodide was used for selecting viable cells. Cell analysis was performed using a LSRII Fortessa, and fluorescence-activated cell sorting (FACS) experiments were done using an AriaII cytometer (BD Biosciences, San Jose, CA). Data were analyzed with FlowJo software (TreeStar, OR).

Phase-contrast μCT imaging and analysis

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To quantify tendon and articular cartilage volume, knee joints were dissected from mice, stained with contrast agents, and scanned by phase-contrast μCT. The articular cartilage volume and surface were analyzed using TriBON software (RATOC, Tokyo, Japan) as previously described (Nixon et al., 2018; Ruan et al., 2013a; Ruan et al., 2013b; Stone et al., 2019). Using this technique, we quantified the patellar tendon volume by examining knee joints in transverse where the patellar tendon boundary was easily distinguished from the joint capsule. Tendon volume was assessed from its origin within the patella to its insertion at the tibia.

Transmission electron microscopy analysis of collagen fibril size

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Mouse ankle and knee joints were dissected and fixed in fresh 1.5% glutaraldehyde/1.5% PFA (Tousimis) with 0.05% tannic acid (Sigma) in 1 × PBS at 4°C overnight to preserve the native tension on relevant tendons. The next day, flexor digitorum longus (FDL), Achilles, and patellar tendons were dissected out in 1 × PBS, and placed back into fixative. Samples were then post-fixed in 1% osmium tetroxide (OsO4), rinsed in Dulbecco’s Modified Eagle Medium (DMEM), and dehydrated in a graded series of ethanol to 100%. Samples were rinsed in propylene oxide, infiltrated in Spurrs epoxy, and polymerized at 70°C overnight. TEM images were acquired using an FEI G20 TEM at multiple magnifications to visualize transverse and longitudinal sections of collagen fibrils. Collagen fibril diameter was measured using the Fiji release of ImageJ (Schindelin et al., 2012).

Tendon biomechanical testing

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Biomechanical tests were performed in tension on a universal testing machine (Instron 5848 Microtester) using a 100N load cell. The tests were performed under displacement control, at a rate of 0.1 N/s, until failure. Data was collected at 40 Hz, and stiffness and ultimate loads were calculated from the load-displacement curve. Tendons were fixed in the machine using a modification of the clamping technique proposed by Probst and colleagues (Probst et al., 2000). The calcaneus was wedged into a conical slot created in a smooth plastic block, which was formed using a moldable plastic (InstaMorph) to ensure all edges were smooth and would not touch or damage the tendon. The origin of the tendon was affixed to the testing machine using a similar technique to that proposed by Probst. Testing was not performed in a water bath, but rather the tendons were kept moist with application of saline during each test, which lasted less than 60 s.

Tendon collagen cross-linking analysis

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Collagen hydroxylysyl-pyridinoline (HP) cross-links were quantified as previously described (Eyre, 1987; Hudson et al., 2018). In brief, tendons isolated from hindlimbs were hydrolyzed by 6M HCl for 24 hr at 108°C. Dried samples were then dissolved in 1% (v/v) n-heptafluorobutyric acid for quantitation of HP by reverse-phase HPLC with fluorescence monitoring.

RNA-seq analysis

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At 1 month-of-age, Achilles tendons were excised using scissors proximal to the calcaneal insertion and distal to the tendon-muscular-junction, whereas patellar tendon were removed via scalpel just proximal to the tibial insertion and distal to the patella. Tendons were not cleaned of their paratenon layers in either case. RNA extraction for both tissues was performed with the Fibrous Connective Tissue kit (Qiagen), with columns from the RNeasy Micro Kit (Qiagen) employed for the patellar tendon. Quality control, library preparation, sequencing, and differential gene expression analysis including gene ontology analysis was performed by GENEWIZ (South Plainfield, NJ). For the examination of predicted Upstream Regulators, we utilized the Ingenuity Pathway Analysis (IPA) platform (Qiagen) with an adjusted p-value of 0.05. The expression is shown as Base Means and read counts of genes were normalized per million transcripts (Transcripts Per Million; TPM).

qRT-PCR analysis

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At 1 month-of-age, Achilles tendons were excised from the calcaneus, immediately distal to the tendon-muscular-junction. RNA was extracted using the Fibrous Connective Tissue kit (Qiagen). qRT-PCR was performed on the LightCycler 96 System (Roche) using gene-specific primers and FastStart SYBR Green I (Roche) following cDNA synthesis with iScript (Bio-Rad). The sequences of primers used were as follows: Crtap fwd: 5’-GCTCTTTGACCAGAGTGACAGG-3’; Crtap rev: 5’-TCCTTCTGGAGCGTCGTCACAT-3’; Col1a1 fwd: 5’-TTGGGGCAAGACAGTCATCGAAT −3’; Col1a1 rev: 5’-TTGGGGTGGAGGGAGTTTACACGAA-3’; Col1a2 fwd: 5’-AACCCATGAACATTCGCAC-3’; Col1a2 rev: 5’-AACTCTCATTGGGATGGTCTACAC-3’; Col2a1 fwd: 5’- GCTCATCCAGGGCTCCAATGATGTAG-3’; Col2a1 rev: 5’- CGGGAGGTCTTCTGTGATCGGTA-3’; Col3a1 fwd: 5’-GACCAAAAGGTGATGCTGGACAG-3’; Col3a1 rev: 5’-CAAGACCTCGTGCTCCAGTTAG-3’; Col9a2 fwd: 5’-CACCAGGCATTGATGGCAAGGA-3’; Col9a2 rev: 5’-AGGACCTCCTTTTGTTCCAGGC-3’; Tnc fwd: 5’-GAGACCTGACACGGAGTATGAG-3’; Tnc rev: 5’-CTCCAAGGTGATGCTGTTGTCTG-3’; Lum fwd: 5’-CCTTGGCATTAGTCGGTAGTGTCAGT-3’; Lum rev: 5’-CGATTTGGTTATTCCTCAGGTAAAG-3’; Tnmd fwd: 5’- CTTTACTAGGCTACTACCCATACCCCTACT-3’; Tnmd rev: 5’- ATATATTGGCTAACAGAAGGTTAAGCGTTT-3’; Fn1 fwd: 5’-CCCTATCTCTGATACCGTTGTCC-3’; Fn1 rev: 5’-TGCCGCAACTACTGTGATTCGG-3’; Fbn1 fwd: 5’-AGCCAGAACCTTCACATCATGGTACAAT-3’; Fbn1 rev: 5’- AGCACCAAACAGACAACAGAAACCTA-3’; Thbs3 fwd: 5’-GACCAGTGTGATGACGATGCTG-3’; Thbs3 rev: 5’-ACAGTTGTCGCAGGCATCACCA-3’; Scx fwd: 5’-AAGACGGCGATTCGAAGTTAGAAG-3’; Scx rev: 5’-TCTCTCTGTTCATAGGCCCTGCTCATAG-3’; Mkx fwd: 5’-CAAGGACAACCTCAGCCTGAGA-3’; Mkx rev: 5’-CGGTGCTTGTAAAGCCACTGCT-3’; Egr1 fwd: 5’-AGCGAACAACCCTATGAGCACC-3’; Egr1 rev: 5’- ATGGGAGGCAACCGAGTCGTTT-3’; CD31 fwd: 5’- CCAAAGCCAGTAGCATCATGGTC-3’; CD31 rev: 5’- GGATGGTGAAGTTGGCTACAGG-3’.

Immunohistochemistry

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Immunohistochemistry was performed using anti-αSMA (Abcam, ab5694, 1:200), anti-MMP2 (R and D Systems, AF1488, 1:400), and anti-phospho-NFκB p65 (Ser536) (Cell Signaling (93H1), #3033, 1:20) antibodies. Briefly, slides of knee joints from 4 month wildtype and Crtap-/- mice were deparaffinized and treated with 3% hydrogen peroxide and proteinase K solution (20 mg/ml) for 10 min. Slides were blocked using 5% normal donkey serum and incubated for 1 hr. Primary antibodies were diluted in blocking solution and incubated overnight at 4°C. Slides were washed with PBS and incubated in anti-rabbit-biotin (Jackson Immunoresearch, 711-065-152, 1:400 for αSMA or 1:100 for phospho-NFκB) or anti-goat-biotin (Jackson Immunoresearch, 705-065-147, 1:500 for MMP2) for 1 hr. Following PBS wash, slides were incubated in streptavidin-HRP (Jackson Immunoresearch, 016-030-084, 1:400–500 for αSMA and MMP2 or 1:100 for phosho-NFκB) for 30 min then washed with PBS. Slides were incubated with DAB substrate (Vector Laboratories, SK-4100) for approximately 2 min, counterstained with hematoxylin, then cleared and mounted with a coverslip.

Open-field assessment of spontaneous motor activity

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Open-field activity was measured using the VersaMax Animal Activity Monitoring System (AccuScan Instruments, Columbus, OH). On the day of assessment, mice were transferred to the test room and allowed to acclimate in their home cage for 30 min at 50 Lux of illumination with 60 dB of white noise. Mice were then placed individually into clear 40 cm ×40 cm × 30 cm chambers and allowed to move freely for 30 min. Locomotion parameters and zones were recorded using the VersaMax activity monitoring software. Chambers were cleaned with 30–50% ethanol to remove the scent of previously tested mice between each run.

Rotarod analysis of motor coordination and endurance

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On the day of assessment, mice were transferred to the test room and allowed to acclimate within their home cage for 30 min at 50 Lux of illumination with 60 dB of white noise. Mice were then placed on a rotarod (UGO Basile, Varese, Italy) set to accelerate from 5-to-40 RPM over 5 min. Five trials were performed per day for two consecutive days (trials 1–10) with a rest time of 5 min between trials. Latency to fall was recorded when the mouse fell from the rotating rod or went for two revolutions without regaining control. The rotarod was cleaned with 30–50% ethanol between mice to remove the scent of previously tested animals.

Grid foot slip analysis of motor coordination

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The grid foot slip assay consisted of a wire grid set atop a stand where the movement was recorded by a suspended digital camera. Mice were transferred to the test room on the day of assessment and allowed to acclimate within their home cage for 30 min at 50 Lux of illumination with 60 dB of white noise. Mice were then placed one at a time on the grid and allowed to move freely for 5 min. The observer sat 6–8 feet away at eye-level to the mouse and recorded forelimb and hindlimb foot slips using the ANY-maze video tracking software (Stoelting Co., Wood Dale, IL). After the test, mice were removed to their original home cage. Forelimb and hindlimb foot slips were normalized to the total distance traveled during the test.

Inverted grid analysis of strength and endurance

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On the day of assessment, mice were transferred to the test room and allowed to acclimate within their home cage for 30 min at 50 Lux of illumination with 60 dB of white noise. Mice were then placed in the middle of a wire grid, held approximately 18-in above a cushioned pad, and inverted. The latency to fall for each mouse was recorded. At the completion, mice were returned to their home cage.

Grip strength analysis

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Mice were transferred to the test room on the day of assessment and allowed to acclimate within their home cage for 30 min at 50 Lux of illumination with 60 dB of white noise. Each mouse was then lifted by its tail onto the bar of a digital grip strength meter (Columbus Instruments, Columbus, OH). Once both forepaws had gripped the bar, the mouse was gently pulled away from the meter by its tail at a constant speed until the forepaws were released. The grip (in N of force) was recorded and the procedure repeated twice for a total of three measurements, which were averaged for the final result.

Statistical analysis

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Determination of sample size was based on previous publications. Biological replicates were defined as an individual mouse for each experiment. Respective tendons from the left and right hindlimbs were combined for TEM, collagen cross-linking, tendon progenitor, and RNA-seq analyses. Data are presented as means ± S.D. or min-to-max box and whisker plots with individual data points. For data whose residuals passed the Shapiro-Wilk test for normality, groups of two were compared using unpaired t-tests, and groups of three or more were compared using one-way ANOVA followed by Tukey’s post-hoc tests. For data whose residuals did not have a normal distribution, groups of two were compared using a Mann-Whitney test, and groups of three or more were compared using Kruskal-Wallis followed by Dunn’s post-hoc tests. For the Rotarod assay, where time was a variable, groups were compared using repeated measures two-way ANOVA followed by Tukey’s post-hoc tests. For all tests reported above, statistical analysis was performed using Prism 9.0.1 (GraphPad Software, La Jolla, CA). For all tests, the exact p-value is reported, and a p-value of <0.05 was considered statistically significant.

Data availability

All data generated or analyzed during this study are included in the manuscript and supporting files. Source data files have been provided for Figure 6 that include full lists of differentially expressed genes resulting from RNA-seq analysis of Achilles and patellar tendons from 1- month wild-type and Crtap-/- mice. For each, a list of predicted upstream regulators identified using Ingenuity Pathway Analysis is also included.

References

    1. Primorac D
    2. Anticević D
    3. Barisić I
    4. Hudetz D
    5. Ivković A
    (2014)
    Osteogenesis imperfecta--multi-systemic and life-long disease that affects whole family
    Collegium Antropologicum 38:767–772.
    1. Veilleux LN
    2. Trejo P
    3. Rauch F
    (2017)
    Muscle abnormalities in osteogenesis imperfecta
    Journal of Musculoskeletal & Neuronal Interactions 17:1–7.

Decision letter

  1. Cheryl Ackert-Bicknell
    Reviewing Editor; University of Colorado, United States
  2. Mone Zaidi
    Senior Editor; Icahn School of Medicine at Mount Sinai, United States
  3. Andreas Traweger
    Reviewer; Paracelsus Private Medical University of Salzburg, Austria
  4. Nathanial Dyment
    Reviewer; University of Pennsylvania, United States

In the interests of transparency, eLife publishes the most substantive revision requests and the accompanying author responses.

Acceptance summary:

The data presented provide evidence that loss of Crtap in mice, which is known to affect multiple connective tissues, results in a hypotrophic tendon phenotype. This Crtap null mouse model recapitulates many aspects of a rare form for Osteogenesis Imperfecta, a disease associated with increased low/no trauma fractures, increased risk of tendon ruptures and lax joint. As such the data presented in this paper partially explain the decreased muscle strength and the tendon phenotype seen in this complex human disease. The results of this study will be of interest to those studying pathologies affecting connective tissues in general, and in particular to those engaged in tendon biology research.

Decision letter after peer review:

Thank you for submitting your article "Tendon and motor phenotypes in the Crtap-/- mouse model of recessive Osteogenesis Imperfecta" for consideration by eLife. Your article has been reviewed by 2 peer reviewers, and the evaluation has been overseen by a Reviewing Editor and Mone Zaidi as the Senior Editor. The following individuals involved in review of your submission have agreed to reveal their identity: Andreas Traweger (Reviewer #1); Nathaniel Dyment (Reviewer #2).

The reviewers have discussed the reviews with one another and the Reviewing Editor has drafted this decision to help you prepare a revised submission.

As the editors have judged that your manuscript is of interest, but as described below that additional experiments are required before it is published, we would like to draw your attention to changes in our revision policy that we have made in response to COVID-19 (https://elifesciences.org/articles/57162). First, because many researchers have temporarily lost access to the labs, we will give authors as much time as they need to submit revised manuscripts. We are also offering, if you choose, to post the manuscript to bioRxiv (if it is not already there) along with this decision letter and a formal designation that the manuscript is "in revision at eLife". Please let us know if you would like to pursue this option. (If your work is more suitable for medRxiv, you will need to post the preprint yourself, as the mechanisms for us to do so are still in development.)

Summary:

In this study, the authors conduct an in-depth examination of the tendon and ligament phenotype in Crtap-/- mice, a model of osteogenesis imperfecta. As is seen in patients, these mice present with deficient muscle strength, and you go on to show that this associated with a reduction in tendon size, reduced collagen fibril size and increased collagen cross-linking. In addition, you observed increased tendon cellularity and changes in gene expression in the tendons reflective of increased inflammation. There were many concerns raised in review, specifically about the model. First, this is a global mutant mouse, and it cannot be determined which aspects of the phenotype are due to deficits intrinsic to the tendon and which were secondary to the other musculoskeletal defects. Ideally the phenotype of a conditional knockout should be presented, but if such a model is not available this issue MUST be addressed in detail in the discussion. Second, there was universal concern among the reviewers about the lack of mechanical testing of the tendon tissue as is outlined in greater detail below. Lastly, there was a lively discussion among the reviewers about the perception that these results are preliminary and lack an in-depth investigation. Detailed comments are listed below.

Essential revisions:

1. Please clarify if Crtap-/- mice also display a phenotype in positional (less load-bearing) tendons, such as tail tendons? If a phenotype is mainly seen in load-bearing tendons, this would imply that the altered ECM triggers different responses due to mechanical load (as is outlined in the Discussion section, lines 408f).

2. The manuscript lacks an in-depth characterization of tendon and ligament tissue. Are there any differences in collagen fiber alignment, Collagen I to Collagen III ratio, etc.? Is Crtap actually expressed in tendons in wild type animals? You demonstrated a shift to smaller diameter collagen fibrils in these mice--is this consistent with previous results in bone? How about cross-links? Are the changes in tendon consistent with changes in bone?

3. You performed extensive functional (motor activity, coordination, and strength) and structural (TEM) assays and showed deficits in the Crtap-/- mice. However, material and structural properties would more directly show alterations in tendon function. As was noted, changes in motor/coordination/strength assays could be due in part to tendon phenotype but may also be due to muscle weakness and pain response. The decreased volume and collagen fibril size with increased cross-links suggests that biomechanical properties will likely be altered but these measures don't always correlate with mechanics. Tendon mechanical tests would be a great addition to the paper (e.g. Young's modulus, max. tensile stress).

4. Lines 258-59: Although Crtap-/- mice display a clear tendon phenotype, you did not investigate tendon development per se. The data merely implies that tendons do not mature properly, as no late embryonic and early postnatal stages have been investigated. The data provided do not allow for a specific conclusion to be made in this regard.

5. Lines 260ff: Based on the data provided it remains questionable if loss of Crtap in tendons is mechanistically responsible for the observed changes in cell density. Only very little data on cell characterization is provided, e.g. you do not investigate the expression of tendon-related markers (i.e IF for Tnmd, Scx, Mkx, Egr1) in situ. Further, a more detailed in vitro characterization of tendon stem and progenitor cells (TDSPCs) isolated from Crtap-/- tendon tissue would further substantiate this claim (e.g. proliferation rate, trilineage differentiation potential, etc.)

6. Although the result from RNASeq analysis are interesting, you do not verify any of their findings by independent means. At a minimum, a change in expression of the identified candidate genes should be demonstrated by qPCR and/or Western blot. Further, mechanistic insight for any of biological processes shown to be impacted by the loss of Ctarp-/- should be provided.

7. You provide results from several behavioral tests clearly demonstrating motor deficits. Surprisingly, none of test performed allow any conclusions to be drawn on the functional consequences of the tendon phenotype observed. Do the animals actually show any change in gait and/or endurance?

8. There is the claim that the behavioral changes observed can be related to the tendon phenotype. While this is a possibility, did you consider that abnormal muscle forces in part drive the tendon phenotype? Could it be that simply the reduced movement (due to pain) and loading of tendons are (mainly) causative for the observed tendon phenotype? This is actually suggested by the open field test results (Figure 6A/B).

9. Since collagen assembly and organization are disrupted in this model and with many OI models leading to increased bone remodeling, there is reason to be believe that OI tendons may be in a chronic healing response. The apparent increase in the number of CD31+ and CD45+ cells (Figure 2A-B), differential gene expression, and the extreme elongation of the patellar tendon that could be caused, in part, by microtears in the matrix, help to support this hypothesis. It would be interesting to stain for CD31 to see if there is an increased in vascularity or stain for matrix proteins that are elevated in healing or tendinopathic tissue (e.g., TNC, type III collagen, α SMA). A discussion of this mechanism is warranted.

10. Resident tendon progenitor populations are not well understood. While CD146 and CD200 may be markers of progenitors, related to my previous point, production of these proteins is likely increased in healing tissues and may not be specifically expressed in a progenitor population. We would caution labeling the CD146+/CD200+ cells as progenitors and the CD146-/CD200+ cells as immature cells without additional functional assays.

11. The patellar ligament should be referred to as the patellar tendon. Anatomically, the patellar tendon connects two bones but structurally and functionally it is a tendon. It functions in the extension mechanism of the knee and the ECM has less ground substance and is also more aligned than ligaments.

12. It was noted that articular cartilage volume was not altered but did not present quantitative data. We are surprised to not see changes in articular cartilage given prolyl 3-hydroxylation in type II collagen and the role that Crtap may have in this process. In addition, the alterations in subchondral bone and synovial thickening suggest that changes to articular cartilage may also occur.

[Editors' note: further revisions were suggested prior to acceptance, as described below.]

Thank you for resubmitting your work entitled "Tendon and motor phenotypes in the Crtap-/- mouse model of recessive Osteogenesis Imperfecta" for further consideration by eLife. Your revised article has been evaluated by Mone Zaidi (Senior Editor) and a Reviewing Editor.

Summary:

The data presented provide evidence that loss of Crtap in mice, which is known to affect multiple connective tissues, results in a hypotrophic tendon phenotype. This Crtap null mouse model recapitulates many aspects of a rare form for Osteogenesis Imperfecta, a disease associated with increased low/no trauma fractures, increased risk of tendon ruptures and lax joint. As such the data presented in this paper partially explain the decreased muscle strength and the tendon phenotype seen in this complex human disease. The results of this study will be of interest to those studying pathologies affecting connective tissues in general, and in particular to those engaged in tendon biology research.

The manuscript has been improved, but there are some remaining issues, particularly in relation to new data, that need to be addressed, as outlined below:

Essential Revisions:

1. The authors now include biomechanical data which was very much appreciated by the reviewers. However, the authors reported only structural properties (stiffness and max force) but not material properties (modulus and ultimate stress). As the authors also demonstrated that the Achilles tendon was thinner in the mutant mice (Figure 1), it's conceivable that the reduced structural properties could be due to a reduction in cross-sectional area of the tendon. This is only a minor limitation though given the altered ECM seen by TEM but should still be stated.

2. The authors now provide data, that a hypoblastic and hypercellular phenotype is not observed in early postnatal stages. This is an interesting and important finding. While the authors provide quantitative data on the cellularity, no quantitation on patellar tendon diameter is included. This would further underscore their findings.

3. The authors argue that load-bearing tendons in Crtap-/- mice undergo increased remodeling reminiscent of a chronic repair state. Unfortunately, they only provide RT-qPCR to support their claims. As it appears that lack of Crtap renders tendons more sensitive to overload-induced (even at physiological loads) catabolic events, it is important to demonstrate an increase in matrix-remodeling enzymes (e.g. MMPs, etc.), inflammatory events (e.g. expression of pro-inflammatory cytokines, NfkB activation), and fibrotic markers (e.g. α SMA as previously suggested in the prior review) on the protein level (IHC) driving the hypoblastic phenotype. Also, investigating Tgf-b signaling seems warranted. While RT-qPCR data is sometimes helpful the reviewers felt that for some of these issues, histopathological assessment such as IHC for MMPs and/or α-SMA to help validate the injury/healing response would be more informative.

4. Herovicis polychrome stain, which allows some differentiation between ColI/ColIII and also gives more information on the maturity of the tissue. It was felt that this would really strengthen the story being presented in this manuscript.

https://doi.org/10.7554/eLife.63488.sa1

Author response

Essential revisions:

1. Please clarify if Crtap-/- mice also display a phenotype in positional (less load-bearing) tendons, such as tail tendons? If a phenotype is mainly seen in load-bearing tendons, this would imply that the altered ECM triggers different responses due to mechanical load (as is outlined in the Discussion section, lines 408f).

We thank the reviewers for this interesting question. As this manuscript's interest was in examining appendicular load-bearing tendons as they may relate to clinical manifestations in OI patients, such as joint laxity, we did not examine tail tendons in our mice. We have highlighted this fact now in the Discussion of our manuscript (Lines 381-388). In the lab, we have observed that Crtap-/- mice develop kinked tails with incomplete penetrance beginning at 1-2 months-of-age. This is a phenotype we are interested in pursuing in future work in addition to creating a conditional knockout model to address the specificity of the tendon phenotype.

2. The manuscript lacks an in-depth characterization of tendon and ligament tissue. Are there any differences in collagen fiber alignment, Collagen I to Collagen III ratio, etc.? Is Crtap actually expressed in tendons in wild type animals? You demonstrated a shift to smaller diameter collagen fibrils in these mice--is this consistent with previous results in bone? How about cross-links? Are the changes in tendon consistent with changes in bone?

We thank the reviewers for this point. We have added several new analyses and experiments to address these points.

Concerning collagen fibril alignment, we have added longitudinal TEM images to Figure 4 (see Figure 4M-R) that clearly show the irregular organization of collagen fibrils in Crtap-/- mice compared to wildtype (Lines 188-193).

We have also performed qRT-PCR to confirm our RNA-seq data and more closely examine alterations in tendon-specific gene expression in Crtap-/- tendons compared to wildtype. These results highlight that Crtap is expressed in tendon and is absent in tissue from Crtap-/- (Figure 7, Lines 261-276) – a finding that confirms the RNA-seq data in Figure 6.

As part of this new qRT-PCR analysis, we examined the expression of various fibrillar collagens, glycoproteins, SLRPs, tendon transcription factors, and CD31 (as a marker of vascularization). We demonstrate that while a modest reduction in Col1a1 expression is observed with no alteration in Col3a1 expression, there is increased expression of Scx, Tnc, Lum, Tnmd, Fn1, and Thbs3. As the reviewers pointed out below, this increase in tendon marker expression likely indicates that the tendon ECM is undergoing increased remodeling reminiscent of a chronic repair state. This new data is highlighted in Figure 7 and described on Lines 261-276. We discuss these results in the context of the existing literature on tendon maturation and repair on Lines 351-366 of the Discussion.

In the original submission, we discussed how the shift in collagen fibril diameters seen in FDL, Achilles, and patellar tendons from Crtap-/- mice is consistent with mouse models lacking the other two components of the 3-prolyl hydroxylase complex, namely P3h1 and CypB. At the same time, the reviewers bring up an important point regarding whether similarities exist between tendon and bone. To address this, we discuss that while we see increases in HP residues per collagen in Crtap-/- tendons, HP is not drastically changed in Crtap-/- bones; instead, it is a decrease in LP and resulting increase in HP/LP that is seen in bones from Crtap-/- mice. Moreover, there is a complete loss of 3-prolyl hydroxylation at Pro 986 in the chains of type I collagen (see Lines 397-403). Beyond collagen cross-linking, the reductions in ECM and increased cellularity are consistent with that seen in bones, lungs, and glomeruli of these mice (see Lines 328-333).

3. You performed extensive functional (motor activity, coordination, and strength) and structural (TEM) assays and showed deficits in the Crtap-/- mice. However, material and structural properties would more directly show alterations in tendon function. As was noted, changes in motor/coordination/strength assays could be due in part to tendon phenotype but may also be due to muscle weakness and pain response. The decreased volume and collagen fibril size with increased cross-links suggests that biomechanical properties will likely be altered but these measures don't always correlate with mechanics. Tendon mechanical tests would be a great addition to the paper (e.g. Young's modulus, max. tensile stress).

We thank the reviewers for highlighting this point. We have added results from biomechanical testing of Achilles tendons from 1-month-old wildtype, heterozygous, and Crtap-/- mice in the revised manuscript. As is now shown in Figure 1T-U, we observed a significant decrease in the ultimate load and maximum stiffness in Crtap-/- tendons compared to the other two genotypes (see Lines 128-136).

4. Lines 258-59: Although Crtap-/- mice display a clear tendon phenotype, you did not investigate tendon development per se. The data merely implies that tendons do not mature properly, as no late embryonic and early postnatal stages have been investigated. The data provided do not allow for a specific conclusion to be made in this regard.

We thank the reviewers for this important point. In the revised manuscript, we have added a new Figure (see Figure 2) examining the tendon phenotype in Crtap-/- mice at postnatal day 10 (P10). We still observed a slight thinning of the Achilles and patellar tendons at this earlier time point, but there was no increase in cell density in either tendon compared to wildtype. Based on this new data, we conclude that Crtap is required for tendon maturation and postnatal homeostasis but is not likely to be required for their initial formation and development (see Lines 137-142).

5. Lines 260ff: Based on the data provided it remains questionable if loss of Crtap in tendons is mechanistically responsible for the observed changes in cell density. Only very little data on cell characterization is provided, e.g. you do not investigate the expression of tendon-related markers (i.e IF for Tnmd, Scx, Mkx, Egr1) in situ. Further, a more detailed in vitro characterization of tendon stem and progenitor cells (TDSPCs) isolated from Crtap-/- tendon tissue would further substantiate this claim (e.g. proliferation rate, trilineage differentiation potential, etc.)

We thank the reviewers for this important suggestion. As described above for Comment 2, we addressed the concerns regarding tendon-related marker expression by performing qRT-PCR for several of these markers (see Figure 7, Lines 261-276).

In terms of the tendon progenitor cells, the new qRT-PCR data does indeed suggest that changes in CD146+ cells could simply be indicative of a tendon in a chronic but pathologic state of repair. As such, we have de-emphasized the progenitor discussion in the revised manuscript and focused more on the repair hypothesis put forth by the reviewers. That being said, we agree that an interesting avenue for future research would be to examine the properties of the CD146+CD200+ cells identified in Figure 3 to verify if they at all represent a true progenitor population, and to examine how the decrease in CD146+CD200+ population in Crtap-/- mice may (or may not) contribute to the tendon phenotype. We now highlight this important future direction in the Discussion (see Lines 333-337).

6. Although the result from RNASeq analysis are interesting, you do not verify any of their findings by independent means. At a minimum, a change in expression of the identified candidate genes should be demonstrated by qPCR and/or Western blot. Further, mechanistic insight for any of biological processes shown to be impacted by the loss of Ctarp-/- should be provided.

We thank the reviewers for this important suggestion. As described above for Comment 2, we addressed the concerns regarding tendon-related marker expression by performing qRT-PCR for several of these markers (see Figure 7, Lines 261-276).

7. You provide results from several behavioral tests clearly demonstrating motor deficits. Surprisingly, none of test performed allow any conclusions to be drawn on the functional consequences of the tendon phenotype observed. Do the animals actually show any change in gait and/or endurance?

We thank the reviewers for this point. We have tried to clarify in the text what each behavioral test measures. We note that the rotarod assay is an established measure of both motor coordination and endurance. Unfortunately, we did not perform any gait analyses on these mice.

A significant issue in identifying the tendon's contribution to these behavioral metrics is the use of the whole-body Crtap knockout mouse model. In the Discussion of the revised manuscript, we acknowledge that muscle and other tissues may contribute to the phenotype in the Crtap-/- mice (see Lines 422-434). Future work employing a tissue-specific Crtap mouse model will be needed to interrogate this question.

8. There is the claim that the behavioral changes observed can be related to the tendon phenotype. While this is a possibility, did you consider that abnormal muscle forces in part drive the tendon phenotype? Could it be that simply the reduced movement (due to pain) and loading of tendons are (mainly) causative for the observed tendon phenotype? This is actually suggested by the open field test results (Figure 6A/B).

We thank the reviewers for this point and have added a section to the Discussion acknowledging that other tissues, namely muscle, could be contributing to behavioral metrics, including grid foot slip and grip strength (see Lines 422-434). We also discuss that to address such concerns, studies in a tissue-specific model will be required.

9. Since collagen assembly and organization are disrupted in this model and with many OI models leading to increased bone remodeling, there is reason to be believe that OI tendons may be in a chronic healing response. The apparent increase in the number of CD31+ and CD45+ cells (Figure 2A-B), differential gene expression, and the extreme elongation of the patellar tendon that could be caused, in part, by microtears in the matrix, help to support this hypothesis. It would be interesting to stain for CD31 to see if there is an increased in vascularity or stain for matrix proteins that are elevated in healing or tendinopathic tissue (e.g., TNC, type III collagen, α SMA). A discussion of this mechanism is warranted.

This is an excellent point made by the reviewers. We have performed qRT-PCR analysis of Achilles tendons from 1-month-old wildtype and Crtap-/- mice to address this. In addition to the upregulation of many tendon-specific genes (see the explanation for Comment 2), we examined the expression of CD31 at this timepoint and saw no difference between wildtype and Crtap-/- mice. In our tissue sections, we also did not observe any gross vascular infiltration into the tendon body. We agree with the reviewers that the upregulation of tendon markers combined with the changes seen in the ECM organization might indicate that the OI tendons are in a state of chronic healing. We highlight this point now in the Discussion (Lines 331-337, 351-366).

10. Resident tendon progenitor populations are not well understood. While CD146 and CD200 may be markers of progenitors, related to my previous point, production of these proteins is likely increased in healing tissues and may not be specifically expressed in a progenitor population. We would caution labeling the CD146+/CD200+ cells as progenitors and the CD146-/CD200+ cells as immature cells without additional functional assays.

We appreciate the reviewers' comments and acknowledge that the markers for tendon progenitors are not well-established. Indeed, based on the new qRT-PCR data, the changes in CD146+ cells could simply be indicative of a tendon in a chronic but pathologic state of repair. As such, we have de-emphasized the progenitor discussion in the revised manuscript and focused more on the repair hypothesis put forth by the reviewers.

11. The patellar ligament should be referred to as the patellar tendon. Anatomically, the patellar tendon connects two bones but structurally and functionally it is a tendon. It functions in the extension mechanism of the knee and the ECM has less ground substance and is also more aligned than ligaments.

We thank the reviewers for highlighting this error. We have now referred to it as the "patellar tendon" throughout the revised manuscript.

12. It was noted that articular cartilage volume was not altered but did not present quantitative data. We are surprised to not see changes in articular cartilage given prolyl 3-hydroxylation in type II collagen and the role that Crtap may have in this process. In addition, the alterations in subchondral bone and synovial thickening suggest that changes to articular cartilage may also occur.

We thank the reviewers for this point. In Figure 1R-S of the revised manuscript, we have included measurements of articular cartilage volume and surface at 4-months for wildtype, heterozygous, and Crtap-/- mice. In this analysis, we observed no drastic differences between groups (see Lines 121-122). Concerning genetic mouse models of early-onset osteoarthritis, this finding is not surprising as articular cartilage degeneration often occurs at least 6-months postnatally in the absence of a stressor (i.e., trauma).

[Editors' note: further revisions were suggested prior to acceptance, as described below.]

The manuscript has been improved, but there are some remaining issues, particularly in relation to new data, that need to be addressed, as outlined below:

Essential Revisions:

1. The authors now include biomechanical data which was very much appreciated by the reviewers. However, the authors reported only structural properties (stiffness and max force) but not material properties (modulus and ultimate stress). As the authors also demonstrated that the Achilles tendon was thinner in the mutant mice (Figure 1), it's conceivable that the reduced structural properties could be due to a reduction in cross-sectional area of the tendon. This is only a minor limitation though given the altered ECM seen by TEM but should still be stated.

We thank the reviewers for this observation. We have now noted this minor (but important) limitation in the Discussion of our manuscript (Lines 295-298).

2. The authors now provide data, that a hypoblastic and hypercellular phenotype is not observed in early postnatal stages. This is an interesting and important finding. While the authors provide quantitative data on the cellularity, no quantitation on patellar tendon diameter is included. This would further underscore their findings.

We thank the reviewers for this point. While we did not have P10 samples harvested for phase-contrast µCT analysis, we examined differences in tissue diameter by quantifying average tissue area mid-tendon for Achilles and patellar tendons from wildtype and Crtap-/- mice at this age. This data (Figure 2F, Lines 126-128) shows that there was only a slight decrease in mid-tendon area for the Achilles tendon (though not significant), and no difference in mid-tendon area for the patellar tendon between genotypes at P10.

3. The authors argue that load-bearing tendons in Crtap-/- mice undergo increased remodeling reminiscent of a chronic repair state. Unfortunately, they only provide RT-qPCR to support their claims. As it appears that lack of Crtap renders tendons more sensitive to overload-induced (even at physiological loads) catabolic events, it is important to demonstrate an increase in matrix-remodeling enzymes (e.g. MMPs, etc.), inflammatory events (e.g. expression of pro-inflammatory cytokines, NfkB activation), and fibrotic markers (e.g. α SMA as previously suggested in the prior review) on the protein level (IHC) driving the hypoblastic phenotype. Also, investigating Tgf-b signaling seems warranted. While RT-qPCR data is sometimes helpful the reviewers felt that for some of these issues, histopathological assessment such as IHC for MMPs and/or α-SMA to help validate the injury/healing response would be more informative.

We thank the reviewers for highlighting this point and agree that IHC analysis for differences between matrix-remodeling enzymes, inflammatory events, and fibrotic markers would better support out conclusions. We have now performed IHCs for αSMA, MMP2, and phospho-NFκB on patellar tendon sections from 4-month-old wildtype and Crtap-/- mice (Figure 8). Consistent with our RNAseq analysis (Figure 6) and qPCR data (Figure 7), we observed increased levels of all three markers in Crtap-/- mice compared to controls (Figure 8C-H, Lines 252-260).

4. Herovicis polychrome stain, which allows some differentiation between ColI/ColIII and also gives more information on the maturity of the tissue. It was felt that this would really strengthen the story being presented in this manuscript.

As requested by the reviewers, we performed Herovici staining on patellar tendon sections from 4-month-old wildtype and Crtap-/- mice (Figure 8). We now show that there is an increase in immature collagen (indicated by blue staining) in Crtap-/- patellar tendons compared to wildtype (Figure 8A-B, Lines 254-256).

https://doi.org/10.7554/eLife.63488.sa2

Article and author information

Author details

  1. Matthew William Grol

    Department of Molecular and Human Genetics, Baylor College of Medicine, Houston, United States
    Present address
    Department of Physiology and Pharmacology, University of Western Ontario, London, Canada
    Contribution
    Conceptualization, Formal analysis, Validation, Investigation, Visualization, Writing - original draft, Project administration, Writing - review and editing
    For correspondence
    mgrol2@uwo.ca
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-6514-9066

  2. Nele A Haelterman

    Department of Molecular and Human Genetics, Baylor College of Medicine, Houston, United States
    Contribution
    Formal analysis, Validation, Investigation, Writing - review and editing
    Competing interests
    No competing interests declared

  3. Joohyun Lim

    Department of Molecular and Human Genetics, Baylor College of Medicine, Houston, United States
    Contribution
    Formal analysis, Validation, Investigation, Writing - review and editing
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-9670-806X

  4. Elda M Munivez

    Department of Molecular and Human Genetics, Baylor College of Medicine, Houston, United States
    Contribution
    Investigation
    Competing interests
    No competing interests declared

  5. Marilyn Archer

    Department of Orthopaedics and Sports Medicine, University of Washington, Seattle, United States
    Contribution
    Formal analysis, Investigation
    Competing interests
    No competing interests declared

  6. David M Hudson

    Department of Orthopaedics and Sports Medicine, University of Washington, Seattle, United States
    Contribution
    Formal analysis, Investigation, Writing - review and editing
    Competing interests
    No competing interests declared

  7. Sara F Tufa

    Shriners Hospital for Children, Portland, United States
    Contribution
    Formal analysis, Investigation
    Competing interests
    No competing interests declared

  8. Douglas R Keene

    Shriners Hospital for Children, Portland, United States
    Contribution
    Formal analysis, Investigation, Writing - review and editing
    Competing interests
    No competing interests declared

  9. Kevin Lei

    Department of Molecular and Human Genetics, Baylor College of Medicine, Houston, United States
    Contribution
    Investigation
    Competing interests
    No competing interests declared

  10. Dongsu Park

    Department of Molecular and Human Genetics, Baylor College of Medicine, Houston, United States
    Contribution
    Formal analysis, Investigation, Visualization, Writing - review and editing
    Competing interests
    No competing interests declared

  11. Cole D Kuzawa

    Department of Orthopaedic Surgery, UT Health Sciences Center, Houston, United States
    Contribution
    Investigation
    Competing interests
    No competing interests declared

  12. Catherine G Ambrose

    Department of Orthopaedic Surgery, UT Health Sciences Center, Houston, United States
    Contribution
    Formal analysis, Investigation, Writing - review and editing
    Competing interests
    No competing interests declared

  13. David R Eyre

    Department of Orthopaedics and Sports Medicine, University of Washington, Seattle, United States
    Contribution
    Formal analysis, Investigation, Writing - review and editing
    Competing interests
    No competing interests declared

  14. Brendan H Lee

    Department of Molecular and Human Genetics, Baylor College of Medicine, Houston, United States
    Contribution
    Conceptualization, Resources, Formal analysis, Supervision, Funding acquisition, Project administration, Writing - review and editing
    For correspondence
    blee@bcm.edu
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-8573-4211

Funding

Eunice Kennedy Shriver National Institute of Child Health and Human Development (HD024064)

  • Brendan H Lee

Baylor College of Medicine

  • Brendan H Lee

National Institute of Arthritis and Musculoskeletal and Skin Diseases (AR373318)

  • David R Eyre

National Institute of Child Health and Human Development

  • Brendan H Lee

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Ethics

Animal experimentation: This study was performed in strict accordance with the recommendations in the Guide for the Care and Use of Laboratory Animals of the National Institutes of Health. All of the animals were handled according to approved Institutional Animal Care and Use Committee (IACUC) protocols (#AN-1506) at Baylor College of Medicine.

Senior Editor

  1. Mone Zaidi, Icahn School of Medicine at Mount Sinai, United States

Reviewing Editor

  1. Cheryl Ackert-Bicknell, University of Colorado, United States

Reviewers

  1. Andreas Traweger, Paracelsus Private Medical University of Salzburg, Austria
  2. Nathanial Dyment, University of Pennsylvania, United States

Publication history

  1. Received: September 25, 2020
  2. Accepted: May 24, 2021
  3. Accepted Manuscript published: May 26, 2021 (version 1)
  4. Version of Record published: June 8, 2021 (version 2)

Copyright

© 2021, Grol et al.

This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.

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  1. Matthew William Grol
  2. Nele A Haelterman
  3. Joohyun Lim
  4. Elda M Munivez
  5. Marilyn Archer
  6. David M Hudson
  7. Sara F Tufa
  8. Douglas R Keene
  9. Kevin Lei
  10. Dongsu Park
  11. Cole D Kuzawa
  12. Catherine G Ambrose
  13. David R Eyre
  14. Brendan H Lee
(2021)
Tendon and motor phenotypes in the Crtap-/- mouse model of recessive osteogenesis imperfecta
eLife 10:e63488.
https://doi.org/10.7554/eLife.63488

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Research organism

Further reading

    1. Developmental Biology
    2. Genetics and Genomics

    A timer gene network is spatially regulated by the terminal system in the Drosophila embryo

    Erik Clark, Margherita Battistara, Matthew A Benton
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    In insect embryos, anteroposterior patterning is coordinated by the sequential expression of the ‘timer’ genes caudal, Dichaete, and odd-paired, whose expression dynamics correlate with the mode of segmentation. In Drosophila, the timer genes are expressed broadly across much of the blastoderm, which segments simultaneously, but their expression is delayed in a small ‘tail’ region, just anterior to the hindgut, which segments during germband extension. Specification of the tail and the hindgut depends on the terminal gap gene tailless, but beyond this the regulation of the timer genes is poorly understood. We used a combination of multiplexed imaging, mutant analysis, and gene network modelling to resolve the regulation of the timer genes, identifying 11 new regulatory interactions and clarifying the mechanism of posterior terminal patterning. We propose that a dynamic Tailless expression gradient modulates the intrinsic dynamics of a timer gene cross-regulatory module, delineating the tail region and delaying its developmental maturation.

    1. Computational and Systems Biology
    2. Genetics and Genomics

    The potential of integrating human and mouse discovery platforms to advance our understanding of cardiometabolic diseases

    Aaron W Jurrjens, Marcus M Seldin ... Anna C Calkin
    Review Article

    Cardiometabolic diseases encompass a range of interrelated conditions that arise from underlying metabolic perturbations precipitated by genetic, environmental, and lifestyle factors. While obesity, dyslipidaemia, smoking, and insulin resistance are major risk factors for cardiometabolic diseases, individuals still present in the absence of such traditional risk factors, making it difficult to determine those at greatest risk of disease. Thus, it is crucial to elucidate the genetic, environmental, and molecular underpinnings to better understand, diagnose, and treat cardiometabolic diseases. Much of this information can be garnered using systems genetics, which takes population-based approaches to investigate how genetic variance contributes to complex traits. Despite the important advances made by human genome-wide association studies (GWAS) in this space, corroboration of these findings has been hampered by limitations including the inability to control environmental influence, limited access to pertinent metabolic tissues, and often, poor classification of diseases or phenotypes. A complementary approach to human GWAS is the utilisation of model systems such as genetically diverse mouse panels to study natural genetic and phenotypic variation in a controlled environment. Here, we review mouse genetic reference panels and the opportunities they provide for the study of cardiometabolic diseases and related traits. We discuss how the post-GWAS era has prompted a shift in focus from discovery of novel genetic variants to understanding gene function. Finally, we highlight key advantages and challenges of integrating complementary genetic and multi-omics data from human and mouse populations to advance biological discovery.

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    Phenome-wide Mendelian randomization study of plasma triglyceride levels and 2,600 disease traits

    Joshua K Park, Shantanu Bafna ... Ron Do
    Research Article

    Background: Causality between plasma triglyceride (TG) levels and atherosclerotic cardiovascular disease (ASCVD) risk remains controversial despite more than four decades of study and two recent landmark trials, STRENGTH and REDUCE-IT. Further unclear is the association between TG levels and non-atherosclerotic diseases across organ systems.

    Methods: Here, we conducted a phenome-wide, two-sample Mendelian randomization (MR) analysis using inverse-variance weighted (IVW) regression to systematically infer the causal effects of plasma TG levels on 2,600 disease traits in the European ancestry population of UK Biobank. For replication, we externally tested 221 nominally significant associations (p < 0.05) in an independent cohort from FinnGen. To account for potential horizontal pleiotropy and the influence of invalid instrumental variables, we performed sensitivity analyses using MR-Egger regression, weighted median estimator, and MR-PRESSO. Finally, we used multivariable MR controlling for correlated lipid fractions to distinguish the independent effect of plasma TG levels.

    Results: Our results identified 7 disease traits reaching Bonferroni-corrected significance in both the discovery (p < 1.92 × 10-5) and replication analyses (p < 2.26 × 10-4), suggesting a causal relationship between plasma TG levels and ASCVDs, including coronary artery disease (OR 1.33, 95% CI 1.24-1.43, p = 2.47 × 10-13). We also identified 12 disease traits that were Bonferroni-significant in the discovery or replication analysis and at least nominally significant in the other analysis (p < 0.05), identifying plasma TG levels as a novel potential risk factor for 9 non-ASCVD diseases, including uterine leiomyoma (OR 1.19, 95% CI 1.10-1.29, p = 1.17 × 10-5).

    Conclusions: Taking a phenome-wide, two-sample MR approach, we identified causal associations between plasma TG levels and 19 disease traits across organ systems. Our findings suggest unrealized drug repurposing opportunities or adverse effects related to approved and emerging TG-lowering agents, as well as mechanistic insights for future studies.

    Funding: RD is supported by the National Institute of General Medical Sciences of the National Institutes of Health (NIH) (R35-GM124836) and the National Heart, Lung, and Blood Institute of the NIH (R01-HL139865 and R01-HL155915).