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Mechanosignaling activation of TGFβ maintains intervertebral disc homeostasis

  • Bone Research 5, Article number: 17008 (2017)
  • doi:10.1038/boneres.2017.8
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Intervertebral disc (IVD) degeneration is the leading cause of disability with no disease-modifying treatment. IVD degeneration is associated with instable mechanical loading in the spine, but little is known about how mechanical stress regulates nucleus notochordal (NC) cells to maintain IVD homeostasis. Here we report that mechanical stress can result in excessive integrin αvβ6-mediated activation of transforming growth factor beta (TGFβ), decreased NC cell vacuoles, and increased matrix proteoglycan production, and results in degenerative disc disease (DDD). Knockout of TGFβ type II receptor (TβRII) or integrin αv in the NC cells inhibited functional activity of postnatal NC cells and also resulted in DDD under mechanical loading. Administration of RGD peptide, TGFβ, and αvβ6-neutralizing antibodies attenuated IVD degeneration. Thus, integrin-mediated activation of TGFβ plays a critical role in mechanical signaling transduction to regulate IVD cell function and homeostasis. Manipulation of this signaling pathway may be a potential therapeutic target to modify DDD.


Degenerative disc disease (DDD) remains a common musculoskeletal disorder that brings an enormous socioeconomic burden.1,​2,​3 Although numerous factors associated with DDD have been identified, the exact molecular pathogenesis of DDD has yet to be elucidated. The current treatments focus on symptomatic relief from pain through injections, physical therapy, and activity modification4 or surgical intervention such as disc decompression, spinal fusion, and disc replacement.3,5 However, none of these interventions halt the progression of degeneration nor restore the physiologic disc function.

Dysfunction of nucleus pulposus (NP) cells is the key in the onset of intervertebral disc (IVD) degeneration.1,6,​7,​8 It is known that NP cells are of notochord origin,9,​10,​11 termed as notochordal (NC) cells at early age. NC cells are large with intracellular vacuoles making up at least 25% of the cell area.7,8 The large vacuoles generate IVD space during spinal morphogenesis.9,12,​13,​14 During maturation and degeneration, the NC cells undergo morphologic and functional transition with the loss of their vacuoles. The resultant fibroblast-like cells have decreased the expression of extracellular matrix protein such as aggrecan,15 which enables the NP to maintain height and turgor against compressive loads via its osmotic properties.16,17 The mechanism driving NC cell transition is unclear, particularly how the mechanical load influences cell signaling.

Temporal–spatial activation of latent matrix transforming growth factor beta (TGFβ) has been shown to modulate chondrocyte anabolic activity in articular cartilage, maintain bone homeostasis during bone remodeling, and help with tissue repair.18,19 The αv integrins in combination with -β6, -β5, and -β8 have been shown to mediate the activation of TGFβ.20,​21,​22,​23,​24 Integrins enable cells to transduce mechanical loads into biological signaling. As NP cells express αv and multiple β integrin subunits, integrin-mediated activation of TGFβ may play a critical role in IVDs.25 In addition, active TGFβ is known to act upstream of connective tissue growth factor (CTGF/CCN2) and aggrecan, both of which are involved in DDD development.26,27 Thus, we sought to understand the role of TGFβ in IVD homeostasis.

In this study, we systematically investigated the role of mechanical stress on the functional transition of NC cells and IVD homeostasis. Utilizing multiple rodent models, we found that mechanical stress resulted in integrin αvβ6-mediated activation of TGFβ. Abnormal stress resulted in excessive TGFβ signaling and accelerated NC cells functional transition. Administration of RGD peptide and neutralizing antibodies against TGFβ and αvβ6 attenuated these changes. On the other hand, conditional knockout of TβRII or αv also impeded NC cells’ transition and caused IVD degeneration by mechanical stimuli. Thus, precise integrin-induced activation of TGFβ is required to maintain IVD cell function and homeostasis.

Materials and methods


Animal models

Lumbar spine instability mouse model

C57BL/6J (male, 8-week old) mice were purchased from Charles River, Wilmington, MA, USA. After anesthetized with ketamine and xylazine, they were operated by resection of the lumbar 3th–lumbar 5th (L3–L5) spinous processes along with the supraspinous and interspinous ligaments to induce instability of lumbar spine.28,29 Sham operations were carried out only by detachment of the posterior paravertebral muscles from the L3–L5 vertebrae. The operated mice were intraperitoneally injected with either TβRI inhibitor (SB-505124, Sigma-Aldrich, St Louis, MO, USA) at a dose of 1 mg·kg−1 (SB group) or the equivalent volume of vehicle (dimethyl sulfoxide; Veh group) once every 2 days. Mice (8-week old) were killed at 0, 1, 2, 4, and 8 weeks after the surgery (n=6 per group).

Caudal spine instability mouse model

The instability of caudal spine was induced by fully depth annular stab and NP removal of the caudal 7th–8th (C7–8) IVD.30 The adjacent C8–9 IVDs were chosen for observation at 4 weeks post surgery (n=6 per group). The treatments were the same as those described in the first model.

Rat caudal IVD compression model

Twelve-week-old male Sprague–sDawley rats (Charles River) were attached at caudal vertebrae with a loading device.31,​32,​33,​34 In detail, two 0.7366 mm stainless steel Kirchner wires were inserted percutaneously into each of the C8 and C10, and attached to 35 mm external diameter aluminum rings. Rings were pre-coated with a resin and connected longitudinally with four stainless steel threaded rods. Axial loads were applied by four calibrated springs (0.50 N·mm−1) installed over each rod. In the vehicle (Veh) and 1D11 group, the axial stress loaded from the distal side produced a calculated compressive pressure of 1.3 MPa onto C8–9 and C9–10 IVDs through tightening calibrated springs.31,33,34 The C8–9 of loaded IVDs was injected with an alginate bead (1 μL) containing 0.7 μg 1D11 (TGFβ-neutralizing antibody; R&D Systems, Minneapolis, MN, USA),18 whereas the C9–10 IVDs with that containing vehicle (n=6) once during the surgery. In the sham group, the rats were also attached with the loading device at C8 and C10, but no compressive pressure was exerted onto the IVDs. Both C8–9 and C9–10 were injected with vehicle-containing alginate bead. The rats were killed at 2 weeks after the surgery (n=6 per group).

Noto-cre (CD1 background mouse expressing Cre recombinase driven by Noto promoter) mouse strain was obtained from the lab of Cheryle A. Séguin.10 TgfβRIIflox/flox mouse strain (C57BL/6J background mouse homozygous for TgfβRII flox allele) was obtained from the lab of H.L. Moses.35 Notocre::TgfβRIIflox/+ mice were generated by crossing heterozygote Noto-cre strain with homozygote TgfβRIIflox/flox strain. TgfβRII−/− and TgfβRI+/+ (wild-type (WT) littermates) offspring were generated by crossing two Notocre::TgfβRIIflox/+ strains (Notocre::TgfβRIIflox/flox mice that are TgfβRII conditional deletion in Noto lineage cells are referred to as “TgfβRII−/−”. Notocre::TgfβRII+/+ mice that are heterozygous for Noto-cre are referred to as “TgfβRII+/+” in the text, n=6 per group).

The genotype of the mice was determined by PCR analyses of genomic DNA isolated from mouse tails using the following primers: Noto-directed cre forward, 5′- ATACCGGCAGATCATGCAAGC-3′, and reverse, 5′- ATGCACATATGCAACCCACA-3′.10 The loxP TgfβRII allele was identified with the primers forward, 5′- TAAACAAGGTCCGGAGCCCA-3′, and reverse, 5′- ACTTCTGCAAGAGGTCCCCT-3′.36

αvflox/flox mice mouse strain was obtained from the lab of Andrew Burich, Benaroya Research Institute at Virginia Mason. Notocre::αvflox/flox mice that are αv conditional deletion in Noto lineage cells are referred to as “αv−/−”. Notocre:: αv+/+ mice that are heterozygous for Noto-cre are referred to as “αv+/+” in the text (n=3 per group). The loxP αv allele was identified with the primers forward, 5′- TTCAGGACGGCACAAAGACCGTTG-3′, and reverse, 5′- CACAAATCAAGGATGACCAAACTGAG-3′.

C57BL/6J mice of the following ages: 16.0-day pregnant, 3 days, 1 weeks, 1 month, 2 months, 3 months and 4 months were purchased from Charles River (n=6 per time point).

All animals (rat and mouse) were maintained in the Animal Facility of the Johns Hopkins University School of Medicine. The experimental protocols for both species were reviewed and approved by the Institutional Animal Care and Use Committee of the Johns Hopkins University, Baltimore, MD, USA.

IVD ex vivo compression model

The L1–L5 lumbar IVDs were removed under sterile conditions from 4-week-old C57BL/6J mice. The collected IVDs were organ-cultured in Dulbecco’s modified Eagle’s medium (Invitrogen, Carlsbad, CA, USA) supplemented with 1% penicillin–streptomycin (MediaTech, Dallas, TX, USA) and pretreated with one of the followings: 2 ng·mL−1 of recombinant mouse TGFβ1 (7666-MB-005, R&D, Minneapolis, Minnesota, USA), 5.0 μg·ml−1 of 1D11, 2 μmol·L−1 of RGD peptide (3498, Tocris Bioscience, Burlington, NC, USA), 100 μg·mL−1 of anti-αVβ6-neutralizing antibody (ab77906, Abcam, Cambridge, MA, USA) or Veh (13C4, R&D Systems) overnight. Compression loads of 0 or 1.0 MPa were applied by vertically placing weights on the IVDs after pretreatment. Loading duration was 24 h (n=6 per group).37

We determined the sample size based on power analysis via website (for two groups, 80% power, 5% significance, two-sided), or via G*Power (for more than two groups, 80% power, 5% significance). For animal model and TgfβRII knockout studies, each experiment was conducted twice: one pilot experiment in three samples and two independent experiments of six samples. For αv knockout mice, three independent experiments with six samples were conducted.

Micro Computed Tomography (μCT)

The lower thoracic and whole lumbar spine from mice were dissected, fixed in 10% buffered formalin for 48 h, transferred into phosphate-buffered saline, and then examined by high-resolution μCT (Skyscan1172). The ribs on the lower thoracic were included for the identification of L4–L5 IVD localization. Images were reconstructed and analyzed using NRecon v1.6 and CTAn v1.9 (Skyscan company, San Jose, CA, USA), respectively. Three-dimensional model visualization software, CTVol v2.0 (Skyscan company, San Jose, CA, USA), was used to analyze parameters of the L4–L5 IVD with half height of L4 and L5 vertebrae. The scanner was set at a voltage of 49 kVp, a current of 200 μA, and a resolution of 6.8 μm per pixel to measure the IVD and endplate (EP). A resolution 16.8 μm of per pixel was set for the whole L5 vertebral body measurement. Coronal images of the L4–L5 IVD were used to perform three-dimensional histomorphometric analyses of IVD. IVD volume was defined by the region of interest to cover the whole invisible space between L4 and L5 vertebrae. Parameter: TV (total tissue volume) was used for three-dimensional structural analysis.

Histochemistry, immunohistochemistry, and histomorphometry

The specimens were fixed in 10% buffered formalin for 48 h, decalcified in 10% EDTA (pH 7.4) for 14 days, dehydrated, and embedded in paraffin. Four-micrometer-thick coronal-oriented sections of the L4–L5, C7–9, or C8–10 spine were processed for safranin O and fast green staining. Tartrate-resistant acid phosphatase staining was performed using a standard protocol (Sigma-Aldrich). Immunostaining was performed using a standard protocol. Sections were incubated with primary antibodies to mouse aggrecan (1:200, AB1031, Millipore, Billerica, MA, USA), CCN2 (1:400, ab6992, Abcam), pSmad2/3 (1:200, sc-11769, Santa Cruz, Dallas, TX, USA), integrin αVβ6 (1:100, bs-5791R-Biotin, Bioss, Woburn, MA, USA), integrin αVβ3 (1:100, bs-1310R, Bioss), integrin αVβ5 (1:100, bs-1356R, Bioss), integrin β8 (1:300, ab80673, Abcam), integrin αV (Santa Cruz, 1:100, sc-6617-R), integrin β6 (Santa Cruz, 1:100, sc-6632), and TGFβRII (1:100, sc-400, Santa Cruz) at 4 °C overnight. For immunohistochemical staining, a horseradish peroxidase-streptavidin detection system (Dako, Carpinteria, CA, USA) was subsequently used to detect the immunoactivity, followed by counterstaining with hematoxylin (Sigma-Aldrich). For immunofluorescent assay, the slides were incubated with secondary antibodies conjugated with fluorescence at room temperature for 1 h while avoiding light. Morphometric study was performed by an image autoanalysis system (Olympus DP71, SEG Biological Microscopes, Center Valley, Pennsylvania, USA). Triplicates of each sample were used for staining.

Quantitative histomorphometric analysis

Quantitative histomorphometric analysis was conducted in a blinded manner with Image-Pro Plus Software version 6.0 (Media Cybernetics Inc, Rockville, Maryland, USA). EP and IVD scores were obtained as previously described.1,38 The percentage of pSmad2/3-positive cells was obtained by counting the number of positive staining cells to the number of total cells in the NP region. The expression of integrin αVβ6 was calculated by the sum of integrated optical density in the NP region. The area of CCN2-positive staining was calculated in the whole L4–L5 IVD in lumbar spine instability (LSI) mice (2-month old). In other experiments, the area of CCN2-positive staining was calculated only in the NP region. The percentage of Acan-positive staining was calculated by counting the positive staining area of region of interest that covers all cells in NP.

Quantitative reverse transcription-PCR

Total RNA was extracted from NP tissue of IVD in ex vivo assay using TRIzol reagent (Sigma-Aldrich) according to the manufacturer’s instruction. The yield and purity of RNA were estimated spectrophotometrically using theA260/A280 ratio. Two micrograms of RNA was reverse-transcribed into complementary DNA using the SuperScript first-strand synthesis system (Invitrogen). One microliter of complementary DNA was subjected to quantitative reverse transcription-PCR amplification using SYBR GREENPCR Master Mix (Promega, Madison, WI, USA) and sequence-specific primers for Acan: 5′- CAGATGGCACCCTCCGATAC-3′and 5′- GACACACCTCGGAAGCAGAA-3′. The value of gene expression was normalized relative to the mouse GAPDH: 5′- AATGTGTCCGTCGTGGATCTGA-3′ and 5′- AGTGTAGCCCAAGATGCCCTTC-3′. PCR reactions were performed in triplicates. The data were analyzed using the 2−ΔΔCT method.

Western blot

Western blot analyses were conducted on the protein extraction from NP tissue in ex vivo assay. The protein extraction was centrifuged, and the concentration of supernatants was evaluated by DC protein assay (Bio-Rad Laboratories, Hercules, CA, USA), then the proteins were separated by SDS-polyacrylamide gel electrophoresis and blotted on a polyvinylidene fluoride membrane (Bio-Rad Laboratories). After incubation in specific antibodies, proteins were detected using an enhanced chemiluminescence kit (Amersham Biosciences, Pittsburgh, PA, USA). The target protein concentrations were examined by antibodies recognizing mouse pSmad2 (1:1 000, 3101, Cell Signaling Technology Inc., Danvers, MA, USA), Smad2 (1:1 000, 3103, Cell Signaling Technology Inc.), integrin αV (1:500, sc-6617-R, Santa Cruz), and GAPDH (1:1 000, 8884, Cell Signaling Technology Inc.).


The data were expressed as mean±s.d., and statistical significance was determined using a Student’s t-test in time point or genetic mice comparison, or one-way analysis of variance followed by a post hoc Least-Significance-Difference (LSD) test (homogeneity of variance) or a Tukey’s test (heterogeneity of variance) in treatment or ex vivo assay comparison. The level of significance was defined as P<0.05. All data analyses were performed using SPSS 15.0 analysis software (SPSS Inc, Chicago, Illinois, USA).


Activation of TGFβ associates with reduced NC cell vacuoles and increased extracellular proteoglycan in response to mechanical stress

The IVD height increased in mice from birth through 1 month, and then remained stable before decreasing around 4 months. The NC cells’ sphere-shaped vacuole observed at birth changed to a spindle-like shape by 4 months (Figure 1a and c). Extracellular aggrecan secretion was stimulated on day 3 after birth and accumulated around the NC cells to generate IVD extracellular space adjacent to endplates from day 7 (Figure 1b). To investigate that these changes were associated with mechanical stress, we employed a LSI mouse model by removing spinous processes and posterior supraspinous and interspinous ligaments (Figure 1d).28,29 The effects of mechanical stress on NC cells were analyzed by immunostaining of the IVD sections collected from 2-month-old LSI mice, in which the IVD space is peaked. The vacuole sizes of NC cells gradually decreased beginning at 2 weeks post surgery in LSI, whereas in the sham-operated mice NC size decreased at 4 weeks with Safranin O staining (Figure 1e). Significant IVD degeneration was observed in LSI mice relative to sham-operated mice, as shown by IVD score beginning as early as 1 week post surgery1,38 (Figure 1g). Mechanical stress has been shown to activate latent TGFβ.20,21,39,40 Immunostaining revealed that phosphorylated Smad2/3-positive cells (pSmad2/3+) in the NP were significantly increased 1, 2, and 4 weeks post surgery in the LSI mice relative to the sham controls (Figure 1f and h). Further, the levels of CCN2, a TGFβ downstream factor that upregulates the synthesis of matrix proteins in IVDs,26,27,41,​42,​43 were significantly increased 2 weeks post surgery in LSI mice and gradually decreased to sham control levels by 4 weeks, consistent with the increase of TGFβ activity (Figure 2a–c). Similarly, aggrecan expression, upregulated by CCN2,26,44 was also increased in LSI mice (Figure 2d and e). Taken together, the data reveal that increase of TGFβ activity in response to mechanical stress stimulates secretion of extracellular proteins such as aggrecan. Simultaneously, a reduction in intracellular vacuoles was observed with a transition of IVD space maintained by intracellular vacuoles in early postnatal life versus extracellular matrix in adulthood or with increased mechanical stress.

Figure 1
Figure 1

Mechanical instability induces activation of TGFβ, and reduces NC cell vacuoles. (a) Safranin O-Fast green staining of IVD sections from wild-type mice from E-16.0 to 4 months after birth. (b) Immunostaining of IVD sections showing the expression of aggrecan. n=6 per time point. (c) The height of IVD indicated by the double-headed arrow was measured in a. (d) Lumbar spine instability mouse model (LSI). Mouse L3–L5 spinous processes were resected along with the supraspinous and interspinous ligaments to induce instability of lumbar spine. (This diagram was drawn by the author and has been published in Scientific Reports: (e) Representative Safranin O staining images of the IVD sections showing the changes of NC cells in LSI and sham-operated 2-month-old mice at 0, 1, 2 and 4 weeks (w) post surgery. (f) Representative immunostaining images of IVD sections with antibody against pSmad2/3 (brown). Hematoxylin stains nuclei purple. (g) Evaluation of IVD degeneration by IVD score. (h) Quantification of pSmad2/3+ cells in f. n=6 per group. Data are shown as mean±s.d. *P<0.05, **P<0.01 (two-sided Student’s t test).

Figure 2
Figure 2

Mechanical instability stimulates extracellular aggrecan. (a) Immunofluorescence staining for CCN2 expression (red). DAPI stains nuclei blue. (b) Enlarged images of CCN2 expression in NP, AF and EP at 2 weeks post surgery. (c) Quantification of CCN2 expression in a. (d) Representative images of immunofluorescence staining for aggrecan (Acan, red). DAPI stains nuclei blue. (e) Quantitative analysis of Acan+ area in NC cells. n=6 per group. Data are shown as mean±s.d. *P<0.05, **P<0.01 (two-sided Student’s t test).

Integrin αvβ6 induces TGFβ activation in response to mechanical stress to regulate NC cell function

We then investigated the mechanism of mechanical stress-induced activation of latent TGFβ. The αvβ integrins are one known mechanism that mediates cell-induced conformational change of TGFβ latent complex to release active TGFβ.21,​22,​23,​24,45,46 The αv integrin is the common α subunit for β integrins. Immunostaining of IVD sections revealed that the expression of one specific β integrin, αvβ6, in the NP was significantly increased 2 and 4 weeks post surgery in LSI mice relative to sham control (Figure 3a and b). The pattern of elevation of αvβ6 expression was similar to the increase of pSmad2/3-positive cells (Figure 1f and h), whereas the expression of β8, αvβ5, and αvβ3 did not correlate (Figure 3c–h).

Figure 3
Figure 3

Integrin αVβ6 induces TGFβ activation in response to mechanical stress. (ah) Representative images and quantification of immunostaining of IVD sections with antibodies against (a, b) αVβ6, (c, d) β8, (e, f) αVβ5, and (g, h) αVβ3 (brown) in LSI and sham mice. Hematoxylin stains nuclei purple. n=6 per group. Data are shown as mean±s.d. *P<0.05, **P<0.01 (two-sided Student’s t test). (i) Immunostaining for pSmad2/3 in the NC cells (brown). Hematoxylin stains nuclei purple. (j) Safranin O staining of IVD sections from an IVD ex vivo compression model with application of either Veh (rows 1 and 3), recombinant mouse TGFβ1 (row 2), RGD peptide, TGFβ or αVβ6 neutralizing antibodies (bottom 3 rows). (k) Quantification of pSmad2/3+ cells in i. (l) Western blot analysis of pSmad2 and total Smad2 levels in the IVD. n=6 per group in histological examination. Representative image from three independent experiments were conducted for (l). Data are shown as mean±s.d. *P<0.05, **P<0.01 (ANOVA).

To determine a causal relationship, active TGFβ, RGD peptide, neutralizing antibodies against TGFβ orαvβ6, or vehicle were applied to an ex vivo IVD compression loading model.37 Immunostaining demonstrated that RGD peptide, antibodies against TGFβ (1D11), or αvβ6 all inhibited stress-induced phosphorylation of Smad2/3 in NC cells (Figure 3i and k). The result was confirmed by western blot analysis (Figure 3l). Importantly, the morphology of NC cell vacuoles was altered in the active TGFβ and vehicle-compression treatment groups (Figure 3j, second and third row), whereas the sphere shape of vacuoles was maintained in the RGD, TGFβ (1D11), and αvβ6 antibody groups (Figure 3j, bottom three rows) relative to the zero compression vehicle group (Figure 3j, top row). In contrast, the extracellular CCN2 and aggrecan were significantly stimulated in the active TGFβ group and compression group treated with vehicle (Figure 4a and b, rows 2 and 3; Figure 4c and d) but inhibited in the RGD and TGFβ antibody groups (Figure 4a and b, rows 4 and 5). Messenger RNA expression of aggrecan was similarly inhibited by RGD and TGFβ antibody (Figure 4e).

Figure 4
Figure 4

Mechanical stress regulates NC cell function. (a, b) Immunofluorescence staining of IVD sections for (a) CCN2 and (b) Acan in the NP (red). DAPI stains nuclei blue. (c, d) Quantification of CCN2 and Acan expression in a and b. (e) Expression of Acan mRNA in NP tissues by quantitative RT-PCR (qRT-PCR). n=6 per group in histological examination. Three independent experiments performed in triplicate were conducted for e. Data are shown as mean±s.d. *P<0.05, **P<0.01 (ANOVA).

Conditional knockout of TGFβ type II receptor prohibits functional transition of NC cells

To confirm the role of TGFβ in control of NC cell function in vivo, notochord-originated cell-specific TgfbrII knockout mice (TgfbrII−/−) were generated by crossing floxed TgfbrII mice with Noto-Cre mice. TβRII- and pSmad2/3-positive NC cells were almost undetectable in immunostaining of IVD sections of TgfbrII−/− mice (Figure 5a–d), validating our mouse model. Immunostaining demonstrated that CCN2 and aggrecan were much lower in the NPs of TgfbrII−/− mice relative to WT TgfbrII+/+ littermates (Figure 5e–h), further confirming CCN2 and aggrecan as downstream signaling targets. Safranin O staining of IVD sections showed that NC cells have much larger vacuoles with less proteoglycan in 4-week-old TgfbrII−/− mice relative to their WT TgfbrII+/+ littermates (Figure 5i). Furthermore, the IVD volume was significantly increased in the TgfbrII−/− mice in comparison to their WT TgfbrII+/+ littermates in μCT analysis (Figure 5j). These genetic data demonstrate that TGFβ signaling in NC cells affects vacuole size for IVD morphology.

Figure 5
Figure 5

Conditional knockout of TGFβ type II receptor prohibits functional transition of NC cells. (a, b) Immunostaining of IVD sections from TgfbrII−/− and their TgfbrII+/+ littermates with antibodies against TβRII and pSmad2/3 (brown). Hematoxylin stains nuclei purple. (c, d) Quantification of TβRII- and pSmad2/3-positive cells in a and b. (g, h) Immunofluorescence staining of IVD sections for CCN2 (g) and Acan (h) (red). DAPI stains nuclei blue. (e, f) Quantification of CCN2 and Acan in the NC cells in g and h. (i) Safranin O-fast green staining of L3–4 IVDs in TgfbrII−/− mice and their TgfbrII+/+ littermates (4-week-old). (j) Quantitative analysis of IVD volumes from μCT scan. n=6 per group. Data are shown as mean±s.d. *P<0.05, **P<0.01 (two-sided Student’s t test).

Conditional knockout of integrin αv impedes postnatal functional transition of NC cells

We then examined the role of integrin αv in activation of TGFβ in notochord cells as αv chain is the core to mediate the activation of TGFβ. Floxed αv mice were crossed with Noto-Cre mice to generate αv knockout mice (αv−/−). Immunostaining of IVD sections validated that αv expression was diminished specifically in NC cells, whereas the expression remained unchanged in AF and EP cells in αv−/−mice relative to their WT αv+/+ littermates (Figure 6a). Integrin β6 expression was unaffected in the αv−/− NC cells (Figure 6b). The reduction of αv in the αv−/− NC cells was further confirmed by western blot analysis (Figure 6k). As expected, αvβ6- and pSmad2/3-positive NC cells were significantly reduced in αv−/−mice relative to WT αv+/+ littermates (Figure 6c, d, g and h). The contents of CCN2 and aggrecan were also much lower in the NPs of αv−/− mice relative to WT αv+/+ littermates (Figure 6e, f, i and j). Similar to TgfbrII−/−mice, NC cells had much larger vacuoles with less proteoglycan in the αv−/− mice relative to their WT littermates (Figure 6m). The αv−/− and TgfbrII−/− mice demonstrate that disruption of TGFβ signaling can delay NC morphologic transition. Therefore, to evaluate whether the morphologic change of vacuoles was sufficient to prevent mechanically induced IVD degeneration, we further subjected αv−/− and TgfbrII−/− mice to LSI or sham surgery (Figure 1d). Safranin O staining showed that IVD was significantly degenerated in both LSI αv−/− and TgfbrII−/− mice relative their sham-operated controls (Figure 6n), and demonstrated that complete loss of NC cell TGFβ signaling can also be as detrimental as excessive TGFβ signaling.

Figure 6
Figure 6

Conditional knockout of integrin αv impedes functional transition of NC cells. (a, b) Immunostaining of IVD sections from αv−/− mice and their wild-type αv+/+ littermates (4-week-old) with antibodies against αv (a) and β6 (b) (brown). Hematoxylin stains nuclei purple. (c, d) Immunostaining for pSmad2/3 (c) and αVβ6 (d) in NC cells. (e, f) Immunostaining for CCN2 (e) and Acan (f) in NC cells. (g, h) Quantification of pSmad2/3 (c) and αVβ6 (d) expression in NC cells. (i, j) Quantification of CCN2 (i) and αVβ6 (j) expression in NC cells. (k) Western blot analysis of αv level in NC cells. (l) Western blot analysis of pSmad2 and Smad2 levels in NC cells. (m) Safranin O-fast green staining of L3–4 IVDs showing enlarged vacuoles with less proteoglycans (red orange) in αv−/− mice relative to their αv+/+ littermates (4-week-old). (n) Safranin O staining images of the IVDs from sham-operated or LSI TgfbrII−/− mice and αv−/− mice (8-week-old) at 2 weeks post surgery. n=3 per group. Data are shown as mean±s.d. *P<0.05, **P<0.01 (two-sided Student’s t test).

Inhibition of excess activation of TGFβ attenuates IVD degeneration

We examined whether inhibition of excessive active TGFβ is beneficial for IVD degeneration. TGFβ type I receptor (TβRI) inhibitor (1 mg·kg−1) was intraperitoneally injected in the LSI mice post surgery. Degeneration of IVD was attenuated as assessed by IVD score (Figure 7a). The vacuolar morphology was preserved with the TβRI inhibitor treatment relative to sham-operated versus LSI-operated with vehicle treatment (Figure 7d). As expected, pSmad2/3+ cells were reduced by TβRI inhibitor (Figure 7b and e). Expression of aggrecan and CCN2 was maintained at similar levels of sham-operated mice as opposed to the elevation of both seen in the LSI-operated vehicle-treated group (Figure 7c, f and g).

Figure 7
Figure 7

Inhibition of excess active TGFβ attenuates IVD degeneration in LSI mice. (a) IVD score in sham, LSI mice with injection of either Veh or TβRI inhibitor (SB, 1.0 mg·kg−1). (b, e) Immunostaining and quantification of pSmad2/3 in the NP (brown). Hematoxylin stains nuclei purple. (c) Quantification of CCN2 areas in g. (d) Safranin O staining of L4–5IVD section. (f, g) Immunofluorescence staining of IVD sections for Acan (f) and CCN2 (g) (red). DAPI stains nuclei blue. n=6 per group. Data are shown as mean±s.d. *P<0.05, **P<0.01, #P<0.05, ##P<0.01 (ANOVA).

In parallel, we administrated the TGFβ-neutralizing antibody directly into the IVD in a rat caudal IVD compression model.31,​32,​33,​34 (Figure 8a) Neutralizing active TGFβ in the IVD prevented IVD degeneration as defined by preservation of the NC cells morphology under static compression relative to vehicle treatment (Figure 8c). The expression pSmad2/3+ in the NC cells was reduced with TGFβ antibody treatment compared to vehicle under static compression (Figure 8d and h). Similar results were obtained using a caudal spine instability mouse model by intraperitoneal injection of TβRI inhibitor30,47,48 (Figure 8b), in which IVD degeneration was effectively prevented (Figure 8e–g and 8i–k ).

Figure 8
Figure 8

Inhibition of excess active TGFβ attenuates IVD degeneration in CIC rats and CSI mice. (a, c, d, h) Local administration of TGFβ neutralizing antibody (1D11, 0.7 μg) into the NP of rat caudal IVD compression model (CIC, 12-week-old) prevented IVD degeneration. (a) Rat CIC model. Rats were attached with the loading device. The axial stress loaded from the distal side produced a compressive pressure of 1.3 MPa on C8–9 and C9–10 IVDs. The C8–9 of loaded IVDs were injected with an alginate bead containing 1D11 while the C9–10 IVDs with that containing vehicle. (c) Safranin O staining of Caudal 8th-9th (C8–9) IVD with 1D11 or vehicle treatment. Immunostaining and quantification of pSmad2/3+ cells (d, h) in the NP of CIC rat (brown). Hematoxylin stains nuclei purple. n=6 per group. (b, e g, i k) Caudal SI(CSI) mouse model was induced by full-depth annular stab and NP removal of the C7–8 IVD. (b) CSI mouse model. The instability of caudal spine was induced by full-depth annular stab and NP removal of the C7–8 IVD. The adjacent C8–9 IVDs were chosen for observation. The adjacent C8–9 IVDs were chosen for observation. (e) Safranin O staining of IVD section. Immunostaining of C8–9IVD sections with antibodies against (f) pSmad2/3 and (g) CCN2; (i) IVD degeneration was evaluated by IVD score at 4 weeks post surgery. Quantification of (j) pSmad2/3+ cells and (k) CCN2+ expression in f and g. n=6 per group. Data are shown as mean±s.d. *P<0.05, **P<0.01, #P<0.05, ##P<0.01 (ANOVA). (l) Model showing mechanosignaling activation of TGFβ controls IVD homeostasis.


The initiation of DDD by NP dysfunction is a hot topic in the spinal disease field. NP cells originate from the notochord. During development, NC cells regulate the spinal morphogenesis by control of intracellular vacuoles evenly distributed in the NP to generate intervertebral space.6,10,49,50 After birth, IVDs gradually change their content with a reduction of intracellular vacuoles of NC cells corresponding to increase extracellular proteoglycans.15 Loss of vacuolar NC cells and their morphologic and functional transition are thought as early degenerative changes of IVD.12 However, the mechanism of NC cells transition is not well understood. In this study, we revealed that integrin αvβ6-induced activation of TGFβ controls the functional transition of NC cells in IVDs in multiple rodent models. Active TGFβ reduced intracellular vacuoles of NC cells, but increased extracellular proteoglycans, thereby shifting the burden of mechanical loads from the cells to the extracellular environment.

Mechanical loads are one of the most important etiologies of DDD.50 In normal physiological situations, appropriate mechanical loading produced by body weight and muscle force is necessary to activate TGFβ in the NP to modulate anabolic activity of NC cells and maintain IVD homeostasis, similar to its role in homeostasis of the bone and cartilage.40,51,​52,​53 However, in pathological conditions, as we found in the present study, compression stresses activate excess TGFβ and result in accelerated functional transition of NC cells, leading to pathologic changes of IVD.

Central to this mechanosignal transduction is the activation of TGFβ by integrin αvβ6. Several of integrin α and β chains have been found in IVD involving in cell–matrix interaction.25,54 Integrin α5β1 has recently been shown to be associated with mechanotransduction in IVD cells.55 Mechanical stress has been shown to induce cell cytoskeleton changes, leading to integrin αvβ6 binding to the latent TGFβ complex for its conformational change to allow active TGFβ to bind to its receptor.45 Similarly, we found it is integrin αvβ6 that correlates to active TGFβ signaling pathway and regulates NC cells function by mechanical stimili. TGFβ signaling activates transcription and secretion of CCN2, which in turn binds to CCN2 receptor to stimulate a cascade of changes in extracellular proteoglycan expression.56 Aggrecan, the major proteoglycan in IVD, exerts osmotic pressure to resist compressive loads.57 However, aggrecan also affects the osmotic pressure in the IVD. Besides shifting water from outside the IVD, our study suggests that aggrecan likely also results in a shifting of water from intracellular to extracelluar matrix and leads to NC cells morphologic transition by dehydration.

TGFβ is recognized as an anabolic factor in IVD and has been found to prevent DDD.58 However, high levels of TGFβ1 have also been observed in the IVDs from DDD patients.39,40,59,​60,​61,​62,​63 One group has previously shown that inhibition of TGFβ can prevent DDD, which was attributed to a change in pSmad1/5/8 to pSmad 2/3 downstream signaling.64 The various effects of TGFβ are likely related to the concentration of TGFβ. Our results demonstrated that pathologic mechanical loading on the spine drove aberrant overactivation of TGFβ, resulting in DDD. Complete inhibition of TGFβ signaling in knockout of TβRII or αv mice also caused IVD degeneration by mechanical stimuli. Thus, TGFβ regulates IVD cell function and homeostasis, whereas either high or low concentrations of TGFβ led to DDD development.

DDD is a polygenic disease exacerbated by many different factors.2,16,50,64,​65,​66,​67,​68 In this study, we found that under mechanical stress, αvβ6 integrin is activated and can release TGFβ from its latent form. Activation of TGFβ signaling pathway in multiple mouse models increased the expression of CCN2, which then upregulated aggrecan. High levels of aggrecan likely increase the osmotic pressure of the extracellular environment to result in a shift in vacuole liquid volume, resulting in an apparent change in NC cell morphology, from vacuole-like to fibroblast-like cells (Figure 8l). Reduction of aberrant TGFβ overactivation in the IVDs through modulation of mechanical stress, or inhibition of either αvβ6 or TGFβ signaling, could have therapeutic potential for DDD.


  1. 1.

    , , et al. Classification of age-related changes in lumbar intervertebral discs: 2002 Volvo Award in basic science. Spine 2002; 27: 2631–2644.

  2. 2.

    , , . Lumbar disc degeneration: correlation with age, sex, and spine level in 600 autopsy specimens. Spine 1988; 13: 173–178.

  3. 3.

    . Intervertebral disc: anatomy-physiology-pathophysiology-treatment. Pain Pract 2008; 8: 18–44.

  4. 4.

    , . Medications for acute and chronic low back pain: a review of the evidence for an American Pain Society/American College of Physicians clinical practice guideline. Ann Intern Med 2007; 147: 505–514.

  5. 5.

    , , et al. Comparative charge analysis of one- and two-level lumbar total disc arthroplasty versus circumferential lumbar fusion. Spine 2007; 32: 2905–2909.

  6. 6.

    , , . Notochordal cells interact with nucleus pulposus cells: regulation of proteoglycan synthesis. Exp Cell Res 1999; 246: 129–137.

  7. 7.

    , , . Cytomorphology of notochordal and chondrocytic cells from the nucleus pulposus: a species comparison. J Anat 2004; 205: 357–262.

  8. 8.

    , , . The notochordal cell in the nucleus pulposus: a review in the context of tissue engineering. Tissue Eng 2003; 9: 667–677.

  9. 9.

    , , . Toward an understanding of the role of notochordal cells in the adult intervertebral disc: from discord to accord. Dev Dyn 2010; 239: 2141–2148.

  10. 10.

    , , et al. Tracing notochord-derived cells using a Noto-cre mouse: implications for intervertebral disc development. Dis Model Mech 2012; 5: 73–82.

  11. 11.

    , . Bridging the gap: understanding embryonic intervertebral disc development. Cell Dev Biol 2012; 1: pii: 103.

  12. 12.

    , , . The vacuole within: how cellular organization dictates notochord function. Bioarchitecture 2013; 3: 64–68.

  13. 13.

    , . Hedgehog signaling is required for formation of the notochord sheath and patterning of nuclei pulposi within the intervertebral discs. Proc Natl Acad Sci USA 2011; 108: 9484–9489.

  14. 14.

    , , . Shh signaling from the nucleus pulposus is required for the postnatal growth and differentiation of the mouse intervertebral disc. PLoS ONE 2012; 7: e35944.

  15. 15.

    , , et al. Matrix remodeling during intervertebral disc growth and degeneration detected by multichromatic FAST staining. J Histochem Cytochem 2009; 57: 249–256.

  16. 16.

    , . What is intervertebral disc degeneration, and what causes it? Spine 2006; 31: 2151–2161.

  17. 17.

    , . Mechanobiology of the intervertebral disc and relevance to disc degeneration. J Bone Joint Surg Am 2006; 88 Suppl 2: 52–57.

  18. 18.

    , , et al. Inhibition of TGF-beta signaling in mesenchymal stem cells of subchondral bone attenuates osteoarthritis. Nat Med 2013; 19: 704–712.

  19. 19.

    , , et al. Myofibroblast contraction activates latent TGF-beta1 from the extracellular matrix. J Cell Biol 2007; 179: 1311–1323.

  20. 20.

    , , et al. Targeting of alphav integrin identifies a core molecular pathway that regulates fibrosis in several organs. Nat Med 2013; 19: 1617–1624.

  21. 21.

    , . aV integrins and TGF-beta-induced EMT: a circle of regulation. J Cell Mol Med 2012; 16: 445–455.

  22. 22.

    , , . TGFbeta: a sleeping giant awoken by integrins. Trends Biochem Sci 2011; 36: 47–54.

  23. 23.

    . Integrin-mediated activation of latent transforming growth factor beta. Cancer Metastasis Rev 2005; 24: 395–402.

  24. 24.

    , , et al. The integrin alpha v beta 6 binds and activates latent TGF beta 1: a mechanism for regulating pulmonary inflammation and fibrosis. Cell 1999; 96: 319–328.

  25. 25.

    , , . Integrin expression in cells of the intervertebral disc. J Anat 2004; 204: 515–520.

  26. 26.

    , , et al. Regulation of CCN2/connective tissue growth factor expression in the nucleus pulposus of the intervertebral disc: role of Smad and activator protein 1 signaling. Arthritis Rheum 2010; 62: 1983–1992.

  27. 27.

    , , et al. Impaired intervertebral disc development and premature disc degeneration in mice with notochord-specific deletion of CCN2. Arthritis Rheum 2013; 65: 2634–2644.

  28. 28.

    , , . Experimental cervical spondylosis in the mouse. Spine 1991; 16 (10 Suppl): S495–S500.

  29. 29.

    , , et al. The relationship between apoptosis of endplate chondrocytes and aging and degeneration of the intervertebral disc. Spine 2001; 26: 2414–2420.

  30. 30.

    , , et al. Stab incision for inducing intervertebral disc degeneration in the rat. Spine 2007; 32: 17–24.

  31. 31.

    , . Intervertebral disc cell death is dependent on the magnitude and duration of spinal loading. Spine 2000; 25: 1477–1483.

  32. 32.

    , , et al. Compression-induced degeneration of the intervertebral disc: an in vivo mouse model and finite-element study. Spine 1998; 23: 2493–2506.

  33. 33.

    , . Biological response of the intervertebral disc to dynamic loading. J Biomech 2004; 37: 329–337.

  34. 34.

    , , et al. Matrix metalloproteinase (MMP)-3 gene up-regulation in a rat tail compression loading-induced disc degeneration model. J Orthop Res 2010; 28: 1026–1032.

  35. 35.

    , , et al. Conditional inactivation of the TGF-beta type II receptor using Cre:Lox. Genesis 2002; 32: 73–75.

  36. 36.

    , , et al. TGF-beta type II receptor phosphorylates PTH receptor to integrate bone remodelling signalling. Nat Cell Biol 2010; 12: 224–234.

  37. 37.

    , , et al. Mechanical stress-induced apoptosis of endplate chondrocytes in organ-cultured mouse intervertebral discs: an ex vivo study. Spine 2003; 28: 1528–1533.

  38. 38.

    , , et al. A novel rabbit model of mild, reproducible disc degeneration by an anulus needle puncture: correlation between the degree of disc injury and radiological and histological appearances of disc degeneration. Spine 2005; 30: 5–14.

  39. 39.

    , , et al. [Association of transforming growth factor-beta1 with pathological grading of intervertebral disc degeneration]. Nan Fang Yi Ke Da Xue Xue Bao 2012; 32: 897–900.

  40. 40.

    , , et al. Possible pathogenesis of painful intervertebral disc degeneration. Spine 2006; 31: 560–566.

  41. 41.

    . The Notochord, Notochordal cell and CTGF/CCN-2: ongoing activity from development through maturation. J Cell Commun Signal 2008; 2: 59–65.

  42. 42.

    , , et al. Expression and role of connective tissue growth factor in painful disc fibrosis and degeneration. Spine 2009; 34: E178–E182.

  43. 43.

    , , et al. CCN2 suppresses catabolic effects of interleukin-1 beta(il-1beta) through alpha5beta1 and alphavbeta3 integrins in nucleus pulposus cells: implications in intervertebral disc degeneration. J Biol Chem 2014; 289: 7374–7387.

  44. 44.

    , , et al. CCN2 (connective tissue growth factor) is essential for extracellular matrix production and integrin signaling in chondrocytes. J Cell Commun Signal 2007; 1: 45–58.

  45. 45.

    , . Integrins and the activation of latent transforming growth factor beta1—an intimate relationship. Eur J Cell Biol 2008; 87: 601–615.

  46. 46.

    , , et al. TGF-beta latency: biological significance and mechanisms of activation. Stem Cells 1997; 15: 190–197.

  47. 47.

    . Animal models of intervertebral disc degeneration: lessons learned. Spine 2004; 29: 2742–2750.

  48. 48.

    , , et al. Are animal models useful for studying human disc disorders/degeneration? Eur Spine J 2008; 17: 2–19.

  49. 49.

    , , . Notochord vacuoles are lysosome-related organelles that function in axis and spine morphogenesis. J Cell Biol 2013; 200: 667–679.

  50. 50.

    , , et al. Degeneration and regeneration of the intervertebral disc: lessons from development. Dis Model Mech 2011; 4: 31–41.

  51. 51.

    , , et al. Endogenous TGF-beta activity limits TSLP expression in the intervertebral disc tissue by suppressing NF-kappaB activation. J Orthop Res 2013; 31: 1144–1149.

  52. 52.

    , , et al. Smad3 controls beta-1,3-glucuronosyltransferase 1 expression in rat nucleus pulposus cells: implications of dysregulated expression in disc disease. Arthritis Rheum 2012; 64: 3324–3333.

  53. 53.

    , , et al. Influence of age-related degeneration on regenerative potential of human nucleus pulposus cells. J Orthop Res 2010; 28: 379–383.

  54. 54.

    , , et al. Functional integrin subunits regulating cell-matrix interactions in the intervertebral disc. J Orthop Res 2007; 25: 829–840.

  55. 55.

    , , et al. Functional impact of integrin alpha5beta1 on the homeostasis of intervertebral discs: a study of mechanotransduction pathways using a novel dynamic loading organ culture system. Spine J 2014; 15: 417–426.

  56. 56.

    . CCN proteins: multifunctional signalling regulators. Lancet 2004; 363: 62–64.

  57. 57.

    , . Aggrecan, an unusual polyelectrolyte: review of solution behavior and physiological implications. Acta Biomater 2012; 8: 3–12.

  58. 58.

    , , et al. TGF-beta signaling plays an essential role in the growth and maintenance of intervertebral disc tissue. FEBS Lett 2011; 585: 1209–1215.

  59. 59.

    , , et al. Degenerative grade affects the responses of human nucleus pulposus cells to link-N, CTGF, and TGFbeta3. J Spinal Disord Tech 2013; 26: E86–E94.

  60. 60.

    , , et al. Variations in aggrecan localization and gene expression patterns characterize increasing stages of human intervertebral disk degeneration. Exp Mol Pathol 2011; 91: 534–539.

  61. 61.

    , , et al. Comparison of growth factor and cytokine expression in patients with degenerated disc disease and herniated nucleus pulposus. Clin Biochem 2009; 42: 1504–1511.

  62. 62.

    , , et al. The expression of anabolic cytokines in intervertebral discs in age-related degeneration. Spine 2006; 31: 1770–1774.

  63. 63.

    , , . Expression of fibronectin and TGF-beta1 mRNA and protein suggest altered regulation of extracellular matrix in degenerated disc tissue. Eur Spine J 2005; 14: 17–26.

  64. 64.

    , , et al. Anabolic effects of Peniel 2000, a peptide that regulates TGF-beta1 signaling on intervertebral disc degeneration. Spine 2013; 38: E49–E58.

  65. 65.

    , , . The effects of dynamic loading on the intervertebral disc. Eur Spine J 2011; 20: 1796–1812.

  66. 66.

    , , et al. The lumbar intervertebral disc: From embryonic development to degeneration. Joint Bone Spine 2013; 81: 125–129.

  67. 67.

    , , et al. The pathophysiology of disc degeneration: a critical review. J Bone Joint Surg Br 2008; 90: 1261–1270.

  68. 68.

    , , et al. The molecular basis of intervertebral disc degeneration. Spine J 2013; 13: 318–330.

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We thank the following colleagues for their technical support: Xin Xu, Wenlong Liu, Gehua Zhen, Shouan Zhu, Xiaokai Wang, Changjun Li, Hui Xie and Liang Xie.

Author information


  1. Department of Orthopaedic Surgery, Institute for Cell Engineering, Johns Hopkins University, Baltimore, MD, USA

    • Qin Bian
    • , Lei Ma
    • , Amit Jain
    • , Janet L Crane
    • , Khaled Kebaish
    • , Mei Wan
    • , Paul D Sponseller
    • , Lee H Riley
    •  & Xu Cao
  2. Institute of Spine, Longhua Hospital, Shanghai University of Traditional Chinese Medicine, Shanghai, PR China

    • Qin Bian
    •  & Yongjun Wang
  3. Department of Pediatrics, Johns Hopkins University, Baltimore, MD, USA

    • Janet L Crane
  4. Department of Biomedical Engineering, Columbia University, NY, USA

    • Zhengdong Zhang
    •  & X Edward Guo
  5. Departments of Physiology and Pharmacology, University of Western Ontario, London, Canada

    • Cheryle A Séguin


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The authors declare no conflict of interest.

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Correspondence to Xu Cao.

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