Hexa-D-arginine treatment increases 7B2•PC2 activity in hyp-mouse osteoblasts and rescues the HYP phenotype

Authors

  • Baozhi Yuan,

    1. Department of Medicine, University of Wisconsin-Madison and Geriatric Research and Education Center, William S. Middleton Memorial Veterans Hospital, Madison, WI, USA
    Search for more papers by this author
  • Jian Q Feng,

    1. Department of Biomedical Sciences, Baylor College of Dentistry, Texas A&M Health Science Center, Dallas, TX, USA
    Search for more papers by this author
  • Stephen Bowman,

    1. Department of Medicine, University of Wisconsin-Madison and Geriatric Research and Education Center, William S. Middleton Memorial Veterans Hospital, Madison, WI, USA
    Search for more papers by this author
  • Ying Liu,

    1. Department of Biomedical Sciences, Baylor College of Dentistry, Texas A&M Health Science Center, Dallas, TX, USA
    Search for more papers by this author
  • Robert D Blank,

    1. Department of Medicine, University of Wisconsin-Madison and Geriatric Research and Education Center, William S. Middleton Memorial Veterans Hospital, Madison, WI, USA
    Search for more papers by this author
  • Iris Lindberg,

    1. Department of Anatomy and Neurobiology, University of Maryland Baltimore, Baltimore, MD, USA
    Search for more papers by this author
  • Marc K Drezner

    Corresponding author
    1. Department of Medicine, University of Wisconsin-Madison and Geriatric Research and Education Center, William S. Middleton Memorial Veterans Hospital, Madison, WI, USA
    • 4246 Health Sciences Learning Center, University of Wisconsin School of Medicine and Public Health, 750 Highland Avenue, Madison, WI, 53705, USA.
    Search for more papers by this author

Errata

This article is corrected by:

  1. Errata: Erratum: Hexa-D-arginine treatment increases 7B2•PC2 activity in hyp-mouse osteoblasts and rescues the HYP phenotype Volume 28, Issue 8, 1855, Article first published online: 18 July 2013

Abstract

Inactivating mutations of the “phosphate regulating gene with homologies to endopeptidases on the X chromosome” (PHEX/Phex) underlie disease in patients with X-linked hypophosphatemia (XLH) and the hyp-mouse, a murine homologue of the human disorder. Although increased serum fibroblast growth factor 23 (FGF-23) underlies the HYP phenotype, the mechanism(s) by which PHEX mutations inhibit FGF-23 degradation and/or enhance production remains unknown. Here we show that treatment of wild-type mice with the proprotein convertase (PC) inhibitor, decanoyl-Arg-Val-Lys-Arg-chloromethyl ketone (Dec), increases serum FGF-23 and produces the HYP phenotype. Because PC2 is uniquely colocalized with PHEX in osteoblasts/bone, we examined if PC2 regulates PHEX-dependent FGF-23 cleavage and production. Transfection of murine osteoblasts with PC2 and its chaperone protein 7B2 cleaved FGF-23, whereas Signe1 (7B2) RNA interference (RNAi) transfection, which limited 7B2 protein production, decreased FGF-23 degradation and increased Fgf-23 mRNA and protein. The mechanism by which decreased 7B2•PC2 activity influences Fgf-23 mRNA was linked to reduced conversion of the precursor to bone morphogenetic protein 1 (proBMP1) to active BMP1, which resulted in limited cleavage of dentin matrix acidic phosphoprotein 1 (DMP1), and consequent increased Fgf-23 mRNA. The significance of decreased 7B2•PC2 activity in XLH was confirmed by studies of hyp-mouse bone, which revealed significantly decreased Sgne1 (7B2) mRNA and 7B2 protein, and limited cleavage of proPC2 to active PC2. The expected downstream effects of these changes included decreased FGF-23 cleavage and increased FGF-23 synthesis, secondary to decreased BMP1-mediated degradation of DMP1. Subsequent Hexa-D-Arginine treatment of hyp-mice enhanced bone 7B2•PC2 activity, normalized FGF-23 degradation and production, and rescued the HYP phenotype. These data suggest that decreased PHEX-dependent 7B2•PC2 activity is central to the pathogenesis of XLH. © 2013 American Society for Bone and Mineral Research

Introduction

X-linked hypophosphatemia (XLH) is the archetypal vitamin D–resistant disease in man, characterized by renal phosphate (Pi) wasting with resultant hypophosphatemia, abnormal vitamin D metabolism, defective bone and cartilage mineralization, dentine defects, and stunted growth.1 Using positional cloning techniques, a gene involved in the pathogenesis of XLH was identified2 and designated as “phosphate regulating gene with homologies to endopeptidases on the X chromosome” (PHEX/Phex). Subsequently, more than 280 loss-of-function mutations in PHEX have been reported in patients with XLH.3–6 The murine homologue of the human disease, the hyp-mouse, has a phenotype identical to that evident in patients with XLH, and is due to a large deletion in the 3′ region of the Phex gene.7 These findings suggest that a mutation in the PHEX/Phex gene is responsible for the phenotypic changes both in patients with XLH and the hyp-mouse.

Recent studies have begun to clarify the mechanism(s) that leads to the biochemical and skeletal abnormalities evident in patients with XLH and in the hyp-mouse. Several reports have established that fibroblast growth factor 23 (FGF-23) plays a central role in phosphate homeostasis. Autosomal dominant hypophosphatemic rickets (ADHR) arises from mutations in the gene encoding FGF-23,8 which disrupts the consensus sequence (RXXR) for prohormone convertase (PC)-mediated proteolytic cleavage of FGF-23, resulting in increased circulating levels of the intact biologically active form of the protein.9, 10 In contrast, a distinct set of FGF-23 mutations cause hyperphosphatemic tumoral calcinosis (HPTC) by decreasing either the amount or activity of intact FGF-23.11–16 Finally, transgenic mice overexpressing FGF-23 (under the control of the α1(I) collagen promoter) exhibit growth retardation, osteomalacia, and disturbed phosphate homeostasis, consistent with abnormalities in patients with XLH.17, 18

A central role for FGF-23 in the pathophysiology of XLH has been confirmed by the presence of increased circulating levels of FGF-23 in affected patients19, 20 and in hyp-mice,21 and by reports establishing that the effects of the single phosphatonin, FGF-23, underlie all elements of the characteristic abnormalities comprising the renal and bone phenotype in XLH.21, 22 Moreover, studies in the hyp-mouse have shown that the increased circulating levels of FGF-23 result both from inhibited degradation of full-length FGF-23 to biologically inactive products, and enhanced production of FGF-23, consistent with observations of increased Fgf-23 mRNA.22, 23

Nevertheless, the mechanism(s) by which loss of PHEX function leads to the altered degradation and production of FGF-23 remains unknown. Thus, development of new therapeutic strategies for XLH has been limited and the disease remains incurable. Indeed, the failure of PHEX overexpression in hyp-mice to rescue the phenotype and of FGF-23 antibody treatment to completely resolve the bone mineralization abnormalities in mutant mice highlight the incomplete understanding of the pathophysiological mechanisms regulating FGF-23 degradation and production.24–28

Because FGF-23 is not a PHEX substrate in vivo,29 the increased circulating levels of FGF-23 likely result from a downstream effect of the PHEX/Phex loss-of-function mutations. One potential mechanism by which this may occur is decreased activity of a prohormone convertase (PC), resulting in impaired cleavage at the RXXR motif. Indeed, transfection experiments have revealed that furin effectively cleaves FGF-23,12, 14, 29, 30 although uridine diphosphate-N-acetyl-alpha-D-galactosamine:polypeptide N-acetylgalactosaminyltransferase 3 (GALNT3)-mediated glycosylation near the cleavage site appears to modulate this effect.31, 32 Whether other PCs cleave this precursor has not been examined.

Although a downstream effect of the PHEX/Phex mutation may alter FGF-23 cleavage by limiting the activity of a PC, this effect must also enhance FGF-23 production, to provide complete explanation for the increased serum hormone levels. Previous in vitro studies have documented that dentin matrix acidic phosphoprotein 1 (DMP1), with three potential nuclear localization signals at the carboxy-terminus, localizes as a transcriptional factor to regulate gene expression.33, 34 Moreover, the recent observations that: (1) full-length DMP1 is an inactive precursor and proteolytic processing is an activation step essential to its biological functions; and (2) overexpression of the 57-kDa DMP1 C-terminal fragment in bone rescues the FGF-23 mediated hypophosphatemic rachitic phenotype of the Dmp1 null mouse,35, 36 suggest that alteration of DMP1 degradation may influence FGF-23 production.37, 38 Thus, decreased PC activity due to the PHEX/Phex mutation may also inhibit DMP1 proteolysis, limiting the production of the C-terminal fragment and consequently enhancing Fgf--23 mRNA.

In this work we report the role that PCs play in the pathophysiology of XLH. We demonstrate that PC2 and its binding protein 7B2 are expressed in osteoblasts and that PC2 is a critical enzyme mediating FGF-23 degradation, as well as production, by promoting bone morphogenetic protein 1 (BMP1)-mediated cleavage of DMP1 and thereby altering Fgf-23 mRNA transcription. In addition, we document that both transcription of the Sgne1 (7B2) gene and active 7B2 protein levels are diminished in the hyp-mouse osteoblast, decreasing PC2 enzyme activity and leading to increased serum FGF-23 and the HYP phenotype. Most importantly, we establish that hexa-D-arginine treatment of hyp-mice corrects the abnormal Sgne1 (7B2) transcription and 7B2 protein levels in osteoblasts and normalizes the biochemical phenotype, as well as completely healing the rickets/osteomalacia characteristic of XLH.

Subjects and Methods

Normal and hyp-mice

Normal C57BL/6J mice were mated with C57BL/6J heterozygous hyp-mice (Jackson Animal Laboratories, Bar Harbor, ME, USA) as described.39 Hemizygotic male and heterozygotic female weanling hyp-mice, obtained from the resultant litters, were identified and selected for study, at 2 to 3 weeks of age by genotyping and/or serum phosphorus levels. Equal numbers of male and female normal littermates were chosen for investigation. All mice received a diet containing 0.6% calcium and phosphorus (Teklad Co., Madison, WI, USA) and deionized water ad libitum from the time of weaning until study. Care of mice met or exceeded the standards set forth by the National Institutes of Health in the Guidelines for the Care and Use of Laboratory Animals (NIH publication 86–23, revised 1985). The University of Wisconsin Animal Care and Use Committee approved all procedures. Experimental mice were euthanized by intraperitoneal (i.p.) injection of sodium pentobarbital.

Effects of Decanoyl-Arg-Val-Lys-Arg-Chloromethyl Ketone Administration in Normal Mice

Male and female C57BL/6J mice, aged 6 to 7 weeks, were randomly divided into a control and experimental group with 12 mice per group. At the inception of the study, 6 mice from the control and experimental group were separated for baseline measurements. We administered saline solution or decanoyl-Arg-Val-Lys-Arg-chloromethyl ketone (Dec) 50 µM in saline solution i.p. for 12 days to the remaining control and experimental mice. During the study the mice received the standard diet noted above. For measurements at baseline and termination of the study, mice were euthanized and blood was obtained for assay of serum Pi and FGF-23 levels. Kidneys (1/mouse) were excised for measurement of 25-hydroxyvitamin D [25(OH)D]-1α-hydroxylase enzyme activity, and the remaining kidney and femurs were collected for RNA and protein extraction.

Effects of Hexa-D-Arginine Amide Administration in Normal and hyp-Mice

We assessed the effects of hexa-D-arginine amide (D6R) treatment in normal and hyp-mice. Male and female normal and hyp-mice, aged 3 weeks, were randomly divided into control and treatment groups of at least 8/group. Control and treated mice from each strain received a daily i.p. injection of saline or D6R in saline (1.5 µg/g/day; R&D Biosystems, Emeryville, CA, USA) for 5 weeks. We obtained blood from the retro-orbital plexus daily for measurement of serum Ca and Pi and at day 35 for measurement of FGF-23 levels. Throughout the treatment period, mice received the standard diet noted above and were monitored for changes in behavioral activity and food and water intake to confirm health. All mice received an i.p. injection of Calcein green dye (5 mg/kg; MP Biomedicals, Santa Ana, CA, USA) and Alzarin complexone dye (20 mg/kg; Acros Organics, Fair Lawn, NJ, USA) 8 and 5 days before study termination, respectively. After 5 weeks (3 days following administration of Alzarin) kidneys (1/mouse) were excised for measurement of 25(OH)D-1α-hydroxylase enzyme activity, and the alternate kidneys and femurs (1/mouse) were collected for RNA and protein extraction. The remaining femurs were collected for bone micro–computed tomography (µCT) analysis and bone histomorphometry.

Biochemical measurements

Serum Pi levels were measured using a Phosphorus Liqui-UV kit from Stanbio Laboratory (Boerne, TX, USA), as described.22 Serum calcium levels were assayed using a calcium Liquicolor kit from Stanbio Laboratory following the manufacturer's protocol.22

Serum intact FGF-23 levels were measured using an FGF-23 ELISA kit obtained from Kainos Laboratories (Tokyo, Japan), with antigenic specificity designed to measure the intact molecule. The standard curve and duplicate measurements were obtained following the protocol of the manufacturer. Serum FGF-23 levels were also measured using an ELISA kit, purchased from Immunotops International (San Clemente, CA, USA), with antigenic specificity directed at the C-terminus of FGF-23. Following the manufacturer's protocol, this assay measures both intact FGF-23 and the C-terminal FGF-23 fragments.

Expression Vectors

Fgf-23 expression vector

Full-length mouse Fgf-23 cDNA was subcloned into the mammalian expression vector pcDNA3.1 (Invitrogen, Carlsbad, CA, USA) with a myc-His tag created at the C-terminus. The full-length mouse Fgf-23 cDNA was obtained by PCR (Platinum Pfx Taq; Invitrogen), using a forward primer designed with a KpnI recognition site and a Kozak translational initiation sequence (5′-GGT ACC GCC ACC ATG CTA GGG ACC TG CCT TA-3′), and reverse primer, designed with an XbaI recognition site (5′-TCT AGA GAC GAA CCT GGG AA-3′). The resulting 771-bp product was electrophoresed on a 2% agarose gel, isolated, and purified (Qiagen, Valencia, CA, USA). This blunt-ended product (FGFkzkxba) was subcloned into the pCR-Blunt II-TOPO plasmid (Invitrogen) and was used to transform TOP10 chemically competent E. coli (Invitrogen) (TOPO FGFkzkxba). Transformants were selected using ampicillin (Invitrogen) lysogeny broth (LB) plates and DNAs from resistant colonies sequenced using the M13 Reverse and T7 primers. The cDNA fragment was released using KpnI and XbaI (New England Biolabs, Ipswich, MA, USA), gel purified (Qiagen) and subsequently ligated into the pcDNA 3.1/myc-His A plasmid (Invitrogen) using the LigaFast Rapid DNA Ligation System (Promega, Madison, WI, USA). This plasmid, FGFkzkMyc, was purified and sequenced to confirm that the Fgf-23 cDNA was inserted in-frame with the Myc epitope of the plasmid. A wild-type Fgf-23 cDNA plasmid was also created in the pcDNA3.2/myc-His vector using a reverse primer, designed with an XhoI recognition site (5′-CTC GAG TTC CTC TAC GTG GGC TGA AC-3′) (FGFkzkWT). The PCR product extends through the stop codon of the Fgf-23 gene, thereby stopping transcription of the plasmid before the myc epitope is reached. Initial transfection experiments were done using both FGFkxkMyc and FGFkzkWT and provided similar results, suggesting the myc-His tail of the construct does not interfere with the gene expression and function. Therefore, the transfection experiments were done using FGFkzkMyc (Fgf-23 construct), allowing easy purification of the myc-His tag.

DMP1 expression vectors

The murine full-length Dmp1 coding region was used previously to generate transgenic mice, under the control of a 3.6-kb type I collagen promoter.40 In the current study, the construct was subcloned into the EcoRI site of the expression vector pcDNA3.1 (Invitrogen). The clone was then sequenced to assure proper insertion and correct orientation.

The DMP1 C-terminal 57-kDa construct and mutant DMP1 construct were obtained as described.41 Briefly, based on the cleavage sites identified in rat DMP1, the DMP1 C-terminal 57-kDa construct expressing the 57-kDa fragment was subcloned into an expression vector, containing the 3.6-kb rat type I collagen promoter, plus a 1.6-kb intron 1 at EcoRV and SalI sites, giving rise to the Col1α1-57-kDa construct. The mutant Dmp1 construct was obtained with the DMP1 cleavage site mutated at D197A to resist cleavage.41

Pcsk2 and Sgne1 expression vectors

Mouse full-length Pcsk2 (PC2) and Sgne1 (7B2) cDNA clones (MGC clone ID: 5707923 and 5361810, respectively) were purchased from Invitrogen. The plasmids were transformed into TOP10 chemically competent E. coli (Invitrogen) using selected LB media, following the manufacturer's protocol. The plasmids were collected and purified by a plasmid extraction method (Qiagen), and the size of the insert cDNA was verified by restriction enzyme (NotI and Sal1) digestion, following the recommendations of Invitrogen. The clones were also sequenced to confirm their identity.

Cell culture and in vitro transfection

Immortalized mouse osteoblast (TMob) cells were obtained as described,42 maintained in α modified essential medium (α-MEM), supplemented with 10% fetal bovine serum (FBS), penicillin (100 U/mL), and streptomycin (100 µg/mL), in a humidified atmosphere of 10% CO2, 90% air at 37°C, and split every 3 to 5 days to maintain subconfluence. In preparation for an experiment, cells were plated in six-well plates and grown for 12 to 14 days in α-MEM containing 10% FBS, penicillin, and streptomycin, supplemented with 5 mM β-glycerophosphate and 25 µg/mL ascorbic acid, and the culture medium was changed every 3 days.

Transfection of TMob cells was performed using Lipofectamine 2000 following the manufacturer's suggested protocol (Invitrogen) after optimization of DNA and Lipofectamine ratios. For single transfection studies, cells were cultured in medium until 80% confluent (90% for Sgne1 [7B2] RNAi transfection), and transfected with either a full-length Dmp1, Dmp1 C-terminal construct, mutant Dmp1 construct, or Sgne1 RNAi (Invitrogen). Cells were collected for total RNA and protein extraction 48 hours after the transfection. For triple-transfection studies TMob cells were initially transfected with an Fgf-23 construct and 4 hours later with either Pcsk2 or Sgne1 alone or Pcsk2 plus Sgne1 constructs. After overnight incubation, cells and medium were collected as described earlier in this paragraph.

Analytical Methodology

In vitro assay of murine renal 25(OH)D-1α-hydroxylase activity

We assayed the maximum velocity of renal 25(OH)D-1α-hydroxylase enzyme activity in kidney homogenates by previously described methods.22, 23 Data are expressed as femtomoles 1,25(OH)2D per minute per milligram (wet wt) of kidney.

Real-time–rt PCR assay of mRNA

We performed real-time (RT)-rt PCR assays to quantitate mRNA in bone and kidney from normal and hyp-mice, as well as TMob cells. To isolate total RNA from bone, we euthanized the mice and disarticulated the femurs. The femurs were trimmed of fat and the marrow was removed, prior to freezing in liquid nitrogen for storage at −80°C. To prepare the bone for RNA isolation, samples were homogenized into fine powder in liquid nitrogen using a porcelain mortar and pestle. We extracted the total RNA from the resultant powder, using the TRIzol protocol (Life Sciences Technology, Carlsbad, CA, USA), as described.22 We quantitated Fgf-23, Pcsk2 (PC2), Dmp1, Bmp1, and Sgne1 (7B2) mRNA from the samples following the protocol described22 and using the following gene-specific primers:

  • (Fgf-23, GenBank accession #MC_000072) forward primer: 5′-CTG CTA GAG CCT ATC CGG AC-3′; reverse primer: 5′-AGT GAT GCT TCT GCG ACA A-3′;

  • (Pcsk2 (PC2), GenBank accession #NM_008792) forward primer: 5′-CAC TCC CAA AGA AGG ATG GA-3′; reverse primer: 5′-TAA GAG GCA TTT TGG CTG CT-3′;

  • (Dmp1, GenBank accession #NM_016779) forward primer: 5′-ACT CAC TGT TCG TGG GTG GT-3′; reverse primer: 5′-TTG TGG GAA AAA GAC CTT GG-3′;

  • (Bmp1, GenBank accession #NM_009755) forward primer: 5′-CAC TCC ACA GCA GGA AGT GA-3′; reverse primer: 5′-CTC AGT GAA AGC TCC GGT TC-3′;

  • (Sgne1 (7B2), GenBank accession #NM_009162) forward primer: 5′-PBS-CCC CAA CAT AGT GGC AGA GT-3′; reverse primer: 5′-AAC TGG AAT TCT CGG CTG AA-3′.

We prepared kidney total RNA using the TRIzol reagent.23 Renal Npt2a and Cyp27b1 (25(OH)D-1α-hydroxylase) mRNA were quantitated by RT PCR employing the primers and the protocols described.23

After washing the TMob cells once with 1× PBS, total RNA was extracted, using 1 mL TRIzol reagent per well, and following the manufacturer's protocol.

In all cases the isolated total RNA concentration was measured and the reverse transcription reaction was performed with 5 µg of total RNA, using an iScript First Strand cDNA Kit from Bio-Rad (Hercules, CA, USA). Subsequently, RT-rt PCR was performed, using iTaq SYBR Green Supermix (Bio-Rad), with the specific primers noted above on an ABI 7000 Applied Biosystems Thermocycler (Foster City, CA, USA). GAPDH expression was also determined with each RT-PCR reaction as an internal control for data analyses. Data were collected quantitatively and the CT number corrected by CT readings of the corresponding internal GAPDH controls. Data from a minimum of six determinations (mean ± SEM) are expressed in all experiments as fold changes (relative expression).

Western blot analysis

We performed Western blot analysis to quantify protein concentrations from the bone and kidneys of normal and hyp-mice, as well as TMob cells. Disarticulated femurs, trimmed of all fat and marrow free, were frozen in liquid nitrogen at −80°C prior to homogenization into a fine powder in liquid nitrogen using a porcelain mortar and pestle. Subsequently the powder was transferred into T-PER Tissue Protein Extraction Reagent with Halt protease inhibitor (Thermo Scientific, Rockford, IL, USA). After three 30-second sonications, samples were centrifuged and supernatants were stored at −80°C until use.

Kidneys from the various animal models were rinsed free of blood with ice-cold saline and protein extracts were prepared using a modified protocol as described.23 Briefly, tissues were homogenized in sucrose buffer containing 20 mM HEPES, 1 mM EDTA, 255 mM sucrose, 0.4 mM phenylmethylsulfonyl fluoride, and 2 µg/mL leupeptin. The homogenate was subjected to sonication for 30 seconds and then centrifuged at 1500g for 15 minutes, and the pellet containing mitochondrial protein, including 25(OH)D-1α-hydroxylase, was resuspended in the same buffer, aliquotted, and stored at −80°C until use. The supernatant from the centrifugation, which contained the plasma membrane proteins, was also collected for the measurement of sodium-dependent phosphate transporter 2a (NPT2a) protein.

We prepared protein from TMob cells using the sucrose buffer described in the previous paragraph. In brief, cells in plate wells were washed once with PBS (1×) buffer. Thereafter, the cells were scraped from the plate and the cell suspension was centrifuged at 1500g for 5 minutes, after which the cell pellets were resuspended in the sucrose buffer. The suspension was sonicated for 30 seconds and centrifuged at 1500g for 15 minutes. The resulting cell pellet was again resuspended in the sucrose buffer and stored at −80°C until use.

For preparation of Western blots, a 20-µg aliquot of the protein extracts was electrophoresed in 10% SDS-PAGE gel and transferred to a nitrocellulose membrane. The membrane was washed and probed with an appropriate dilution of specific anti-mouse 25(OH)D-1α-hydroxylase antibody (The Binding Site, Birmingham, UK), anti-human NPT2a antibody (Alpha Diagnostic, International, San Antonio, TX, USA), anti-rat FGF-23 antibody (R&D Systems, Minneapolis, MN, USA), anti-rat DMP1 antibody (from L. Bonewald, University of Missouri–Kansas City, Kansas City, MO, USA), anti-human BMP1 (from D Greenspan, University of Wisconsin–Madison, Madison, WI, USA), or anti-mouse PC2 and anti-mouse 7B2 (Protein Group, Chicago, IL, USA). Subsequently, the membrane was probed with appropriate corresponding secondary antibodies. To quantify the immunoblotting signal, 6 mL of chemiluminescence detection solution (ECL Plus; Amersham, Van Nuys, CA, USA) was added, and the signal was detected by a fluorescence scanner (Storm 860; Amersham). The density of bands was analyzed using ImageQuant 5.2 software (Molecular Dynamics, Sunnyvale, CA, USA). The antibodies were subsequently stripped off by incubation in reprobing solution (62.5 mM Tris-HCL, 2% SDS, and 100 mM 2-mercaptomethanol, pH 6.7) for 30 minutes at 50°C. The membrane was then blocked and probed with specific anti-cytochrome c (for 25(OH)D-1α-hydroxylase protein) or β-actin antibody (for the remaining proteins) to verify the loading equivalence among samples.

In situ hybridization of PC2 and 7B2 in bone

In situ hybridization was performed using a digoxigenin (DIG)-labeled Pcsk2 (PC2) or Sgne1 (7B2) cRNA probe, prepared from a murine Pcsk2 or Sgne1 cDNA fragment with an RNA Labeling Kit (Roche, Indianapolis, IN, USA). The specific cDNA fragment was obtained by PCR using bone total RNA as the template with the following primers:

  • (Pcsk2) forward primer 5′-CAC TCC CAA AGA AGG ATG GA -3′; and reverse primer 5′-CAA CCG TCT TCC CAT TGT CT-3′;

  • (Sgne1) forward primer 5′-GGT TAA AAA TGG CCT CAA GG-3′) and reverse primer 5′-AAC CCA TCC AAT GCT TAT GT-3′).

In situ hybridization was performed on paraffin sections of bone from normal and hyp-mice by previously described methods.35 Briefly, the hybridization temperature was set at 55°C and the excess probe was washed off at a temperature of 70°C. DIG-labeled nucleic acids were detected using an enzyme-linked immunoassay with a specific conjugated anti-DIG-alkaline phosphatase antibody and colored substrates, NBT and BCZP, according to the protocol of the manufacturer (Roche, Indianapolis, IN, USA). Hybridization signals were photographed with a Nikon E800 microscope (Nikon, Tokyo, Japan) and a Magnafine camera (Optronics, Goleta, CA, USA).

Bone Structure and Histomorphology

High-resolution radiography (X-ray) and µCT of femur

Femurs were removed and, after the surrounding muscles were digested, washed in PBS buffer and X-rayed using a Faxitron radiographic inspection unit (Model 8050-020; Field Emission Corporation) with digital image capabilities. To determine the length of the femur, bones were radiographed and the OsteoMeasure system (version 4.1; Atlanta, GA, USA) was used to measure the length from femur head to lateral condyle. Bone samples were also scanned in a µCT imaging system (vivaCT40; Scanco Medical, Bassersdorf, Switzerland) and data were analyzed as described.37

Visualization of bone morphology by Goldner staining

Nondecalcified sagittal sections from femurs were stained using the Goldner-Masson trichrome stain, as reported.35 Sections were photographed using a Nikon microscope at 10× with Bioquant OSTEO v 7.20 software (R&M Biometrics, Nashville, TN, USA). Unmineralized osteoid, staining red-brown, and mineralized bone, staining green, were measured using the Bioquant interactive image analysis system (R&M Biometrics), enabling unbiased sampling, averaging of areas, and determination of the osteoid and mineralized area per total area.

Assessment of bone mineralization dynamics

To assess bone formation and mineral apposition rates, mice were euthanized 3 days after injection of the second fluorescent dye, as noted above in the section entitled Effects of Hexa-D-Arginine Amide Administration in Normal and hyp-Mice. The femurs were removed and fixed in 2% paraformaldehyde and 2.5% glutaraldehyde at room temperature for 4 hours before serial dehydration, as described.35 Sections of 50 µm were cut using a Leitz 1600 saw microtome. To estimate mineralization dynamics, unstained sections were viewed under epifluorescent illumination, using a Nikon PCM-2000 confocal microscope, coupled to an Eclipse E800 upright microscope, and interfaced with Osteomeasure histomorphometry software, version 4.1 (OsteoMetrics, Inc., Decatur, GA, USA).35

Statistical Analysis

Data are expressed throughout as the mean ± SEM. We evaluated the data statistically employing a Student's t test for two-group or treatment comparisons. For multiple group comparison, we used one-way ANOVA, and when a difference was established, the Holm-Sidak method was employed to determine which groups were significantly different. A p value of less than 0.05 was considered statistically significant.

Results

Effects of convertase inhibition in normal C57BL/6J mice

In initial studies, we investigated if a decrease in convertase activity, a potential downstream effect of the PHEX/Phex mutation, results in abnormalities of phosphorus, vitamin D, and FGF-23 homeostasis in normal mice, which are characteristic of the HYP phenotype. Administration of the general convertase inhibitor, Dec, to C57Bl/6J mice for 12 days (50 µM/kg/d i.p.) significantly decreased the serum Pi level (7.20 ± 0.27 versus 5.41 ± 0.10 mg/dL; p < 0.05) (Supplementary Fig. S1A) to values approaching those seen in hyp-mice.22 In contrast, the serum calcium concentration remained unchanged (9.10 ± 0.20 versus 8.93 ± 0.40 mg/dL). The decline in the serum Pi level was due to a commensurate decrease in renal Npt2a mRNA (1.06 ± 0.1 versus 0.69 ± 0.01 relative expression; p < 0.05) and NPT2a protein (0.98 ± 0.02 versus 0.58 ± 0.03 relative expression; p < 0.01) and the likely associated renal Pi wasting (Supplementary Fig. S1A).

Further study revealed that Dec-treated normal mice also exhibited aberrant regulation of renal 25(OH)D-1α-hydroxylase activity (Supplementary Fig. S1B). Thus, whereas the renal Cyp27b1 (25(OH)D-1α-hydroxylase) mRNA (1.04 ± 0.04 versus 1.79 ± 0.05 relative expression; p < 0.01) was significantly increased in Dec-treated mice, consistent with hypophosphatemia, expression of the 25(OH)D-1α-hydroxylase protein (1.02 ± 0.03 versus 0.98 ± 0.06 relative expression) was unchanged compared to untreated animals. Accordingly, 25(OH)D-1α-hydroxylase activity (4.60 ± 0.40 versus 3.70 ± 0.20 fmol/min/mg) was unaltered. These changes reflect the unique translational abnormality in the regulation of vitamin D metabolism previously observed in hyp-mice.23

To establish if the biochemical and metabolic changes observed in the Dec-treated mice occurred through a similar mechanism to that operative in hyp-mice, we studied production and degradation of FGF-23 following treatment (Supplementary Fig. S1C). The serum FGF-23 concentration in treated mice was significantly elevated compared to controls (92.0 ± 8.80 versus 225 ± 14.60 pg/mL; p < 0.01). Moreover, Dec treatment resulted in a significant increase in bone Fgf-23 mRNA (1.00 ± .27 versus 2.3 ± 0.7 relative expression; p < 0.01) and FGF-23 protein levels (0.98 ± 0.03 versus 1.29 ± 0.11 relative expression; p < 0.05). Further in vitro studies confirmed and extended these observations (Supplementary Fig. S1D). Overnight incubation of Dec (25 µM) with TMob cells (mouse osteoblasts) not only enhanced Fgf-23 mRNA (1.2 ± 0.2 versus 6.1 ± 1.5 relative expression; p < 0.01) and full-length FGF-23 protein (1.0 ± 0.2 versus 5.3 ± 0.6 relative expression; p < 0.01), but impaired FGF-23 degradation, as evidenced by Western blots documenting decreased C-terminal FGF-23 fragments in the medium (1.0 ± 0.18 versus 0.07 ± 0.001 relative expression; p < 0.001), despite the increased protein levels. Thus, the emergence of the HYP phenotype in Dec-treated mice was likely dependent on changes in FGF-23 production and degradation, characteristically observed in hyp-mice.22, 23

Convertase Tissue Distribution

Because Dec inhibits the family of proprotein convertases, we examined the expression of the seven known convertases in TMob cells and in normal and hyp-mouse bone to potentially identify the specific enzyme responsible for the putative intracellular degradation and enhanced FGF-23 production in osteoblasts/bone. Furin, PC2, PC4, and PC7 are expressed at the mRNA level in TMob cells (Supplementary Fig. S2A) and in bone samples from normal and hyp-mice (Supplementary Fig. S2B). Additional investigation of murine tissues revealed that furin, PC4, and PC7 are widely expressed in a variety of organs, including brain, lung, heart, liver, spleen, kidney, and skeletal muscle, whereas PC2 is expressed only in the brain and in bone (Supplementary Fig. S2C). Because PC2 cleaves precursor proteins43, 44 and is uniquely colocalized with PHEX in osteoblasts/bone, this convertase was a candidate protein to regulate PHEX-dependent FGF-23 production and cleavage in bone.

Regulation of FGF-23 Cleavage and Production In Vitro

To establish the potential role of PC2 in regulating FGF-23 homeostasis, we initially examined the effects of 7B2 (a chaperone protein required for PC2 activity45), and/or PC2 on FGF-23 cleavage in cultured cells. For these studies we serially transfected TMob cells with Fgf-23, and 4 hours thereafter with Sgne1 (7B2), Pcsk2 (PC2), or Sgne1 and Pcsk2. After incubation overnight, cells were collected for measurement of intact FGF-23, and culture medium for measurement of C-terminal fragments. Western blots revealed that neither 7B2 nor PC2 alone cleaved intact FGF-23 (Fig. 1A). However, transfection with both Sgne1 and Pcsk2 significantly increased the concentration of C-terminal fragments in the culture medium (Fig. 1A). Such increased cleavage likely occurred at the convertase consensus site between amino acids 179 and 180.8–10 These data support the possibility that the 7B2•PC2 complex may play a role in bone FGF-23 metabolism.

Figure 1.

Regulation of FGF-23 cleavage and production by 7B2•SPC2. (A) In TMob cells serially transfected with Fgf-23, and 4 hours thereafter with Pcsk2 (PC2), Sgne1 (7B2), or Signe1 and Pcsk2, Western blots indicate that neither PC2 nor 7B2 alone cleaves intact FGF-23 to its C-terminal fragment. In contrast, the coincident transfection of PC2 and 7B2 cleaves the FGF-23, as evidenced by increased levels of C-terminal FGF-23 fragments in the cells. (B) Transfection of TMob cells with Sgne1 (7B2) RNAi alone revealed that a significant increase in the Fgf-23 mRNA occurs in the TMob cells, contributing to the presence of increased intact FGF-23. (C) Further analysis revealed that the diminished Sgne1 mRNA and 7B2 protein resulted in a significant increase in the intact FGF-23 protein, but a significant decrease in the C-terminal FGF-23 in the culture medium, consistent with the anticipated diminished degradation of FGF-23 due to decreased 7B2•PC2 activity.

Subsequently, to define a potential role for 7B2 and PC2 in the production of Fgf-23 mRNA, we singularly transfected TMob cells with Sgne1 (7B2) RNAi or a Sgne1 (7B2)-encoding expression vector. Forty-eight hours after transfection with Sgne1 RNAi, Fgf-23 mRNA increased significantly (Fig. 1B). In accordance with the increased production of Fgf-23 mRNA, the culture medium from transfected cells exhibited increased FGF-23 protein, but a decreased level of the FGF-23 C-terminal fragment, consistent with inhibited protein degradation (Fig. 1C). In contrast, transfection of TMob cells with a Sgne1 (7B2) expression vector resulted in a significant decrease in Fgf-23 mRNA (1.05 ± 0.0001 versus 0.59 ± 0.11 relative expression; p < 0.01) and a decrease in the level of intact FGF-23 (1.0 ± 0.2 versus 0.63 ± 0.1 relative expression; p < 0.05).

To explore whether the 7B2•PC2 regulation of Fgf-23 mRNA production involves DMP1,36–38 we assessed if DMP1 regulates FGF-23 production in osteoblasts. Initially, we transfected TMob cells with normal or mutated Dmp1-expression vectors. Overexpression of DMP1 reduced Fgf-23 mRNA, while overexpression of proteinase-resistant mutant DMP-1 had no impact (Fig. 2A). Consistent with these observations, transfection of TMob cells with the C-terminal DMP1 fragment (57 kDa) resulted in significantly reduced Fgf-23 mRNA production (Fig. 2A). These data suggest that DMP-1 cleavage and production of the C-terminal fragment may regulate Fgf-23 mRNA production.

Figure 2.

DMP1 regulation of FGF-23 in osteoblasts. (A) Transfection of TMob cells with normal Dmp1, and resultant overexpression, reduced Fgf-23 mRNA expression significantly. In contrast, transfection of TMob cells with proteinase resistant Dmp1 had no effect on Fgf-23 mRNA expression in the TMob cells, suggesting that DMP1 proteolysis is essential to regulate Fgf-23 mRNA production. In accord, transfection of TMob cells with the C-terminal DMP1 fragment significantly decreased Fgf-23 mRNA expression, supporting the role of DMP1 proteolysis in regulation of Fgf-23 mRNA. (B) Serial transfection of TMob cells with Dmp1 and Pcsk2 (PC2) and Sgne1 (7B2) resulted in Western blot evidence of a significant increase in C-terminal and N-terminal DMP1 fragments, and a consequent decrease in the intact DMP1, consistent with 7B2•PC2 mediation of DMP1 proteolysis as a possible factor in regulation of Fgf-23 mRNA production. (C) Transfection of TMob cells with Sgne1 RNAi had no effect on Dmp1 mRNA production, but resulted in a significant decrease in the C-terminal and N-terminal DMP1 fragments, and a consequent increase in the intact DMP1, consistent with diminished proteolysis, further supporting a role for DMP1 cleavage in 7B2•PC2 regulation of Fgf-23 mRNA production. (D) Transfection of TMob cells with Sgne1 (7B2) RNAi had no effect on Bmp1 mRNA, when compared to controls, but did result in a significant decrease in active BMP1 and a resultant increase in Pro-BMP1, changes consistent with 7B2•PC2 mediated activation of BMP1 serving as the mechanism that regulates DMP1 degradation.

Subsequently, we examined whether Sgne1 (7B2) and Pcsk2 (PC2) expression regulates DMP1 cleavage in osteoblasts. Serial transfection of TMob cells with the Dmp1 and Sgne1 and Pcsk2 expression vectors resulted in increased levels of N- and C-terminal DMP-1 proteolytic fragments, and in accord a decrease in intact DMP1 (Fig. 2B). In agreement with these findings, transfection of TMob cells with Sgne1 RNAi, although having no effect on Dmp1 mRNA, significantly increased the intact DMP1 due to a decrease in the levels of the DMP-1 N- and C-terminal cleavage products compared to that in controls (Fig. 2C).

Although these studies indicate that 7B2-dependent PC2 activity may regulate Fgf-23 mRNA expression by altering DMP-1 cleavage, proteolytic processing of DMP-1 occurs at a site that is not a known substrate for PC2. Indeed, the only known enzyme that cleaves DMP-1, exclusively to the C-terminal 57-kDa carboxy-terminal and 37-kDa amino-terminal fragments, is BMP1, a tolloid-like proteinase that is activated by PC-mediated removal of an N-terminal prodomain.46, 47 Thus, we extended our studies to determine whether the 7B2-regulated PC2 activity cleaves the N-terminal prodomain of BMP1. Transfection of TMob cells with Sgne1 RNAi had no effect on pro-Bmp1 mRNA, but decreased the levels of active BMP1 and as a result significantly increased proBMP1 levels (Fig. 2D), consistent with 7B2•PC2-mediated cleavage of proBMP1 to active BMP1. Collectively, these findings support the possibility that PC2, in association with its binding protein 7B2, directly affects both degradation of the intact FGF-23 protein, and indirectly affects regulation of Fgf-23 mRNA, by controlling proBMP1 cleavage to active BMP1 and the downstream proteolytic cleavage of the transcriptional regulator DMP-1.

Expression of 7B2 and PC2 in hyp-Mouse Bone

To confirm a role for 7B2 and PC2 in the regulation of FGF-23 in hyp-mice, we explored if decreased 7B2•PC2 activity was present in the bones from mutant mice, due to decreased expression of 7B2 and/or PC2. In situ hybridization studies documented a significant decrease in Sgne1 (7B2) mRNA in the bones from hyp-mice and comparable levels of Pcsk2 (PC2) mRNA in bones from normal and mutant mice (Fig. 3A). These results were confirmed by measurement of Sgne1 and Pcsk2 mRNA by RT PCR in normal and hyp-mouse bone samples (Fig. 3B). In accord, Western blots revealed decreased pro-7B2 and active 7B2 in hyp-mouse bone (Fig. 3C). Moreover, consistent with the requirement of 7B2 to generate active PC2, in part through proteolysis,45, 48 blots revealed that hyp-mouse bone exhibited a significantly increased proPC2 and decreased active PC2 content (Fig. 3C). Collectively, these data suggest that decreased Sgne1 mRNA and protein in the bones of hyp-mice result in failure to normally cleave proPC2, and diminished 7B2•PC2 activity.

Figure 3.

Expression of 7B2 and PC2 in the bones from normal and hyp-mice. (A) In situ hybridization studies documented that the brown-staining Sgne1 (7B2) mRNA was present in abundance in the bone sections from normal mice, but was clearly substantially decreased in the bone sections from hyp-mice; in contrast, no apparent difference in the Pcsk2 (PC2) mRNA was detectable in bone sections from normal and hyp-mice. (B) Consistent with the observations made by in situ hybridization, real-time PCR measurements revealed significantly less Sgne1 mRNA in hyp-mouse than in normal mouse bone samples, whereas no difference in Pcsk2 mRNA was found. (C) In accord, assessment of 7B2 protein content in the bone samples, employing Western blots, documented significantly less pro-7B2 and active 7B2 protein in the hyp-mouse than in the normal bone samples. In the presence of diminished active 7B2 and consequent decreased PC2 proteolysis, the Western blots revealed significantly increased pro-PC2 content in the hyp-mouse bone and decreased mature PC2.

The decreased 7B2•PC2 activity in hyp-mouse bone was accompanied by a profound increase in the serum FGF-23 concentration (Fig. 4A), resulting from increased Fgf-23 mRNA in the hyp-mouse bone (Fig. 4B) and decreased degradation (Fig. 4C). Consistent with in vitro studies, the mechanism underlying the increased Fgf-23 mRNA was suggested by the presence of normal Bmp1 mRNA in the bones of hyp-mice, but Western blot evidence of significantly increased proBMP1 and decreased active BMP1 levels (Fig. 4D), likely due to the diminished 7B2•PC2 activity. In accord, Dmp1 mRNA was no different from normal in the hyp-mouse bone, but Western blots revealed increased levels of intact DMP-1, due to limited Bmp1-mediated degradation, as evidenced by decreased levels of N- and C-terminal DMP-1 cleavage products in the bones from mutant mice (Fig. 5E). These data are consistent with the hypothesis that decreased 7B2•PC2 activity in hyp-mouse bone increases circulating levels of FGF-23 by limiting cleavage directly, and by increasing Fgf-23 mRNA indirectly, via the BMP1-DMP1 pathway (Supplementary Fig. S2).

Figure 4.

Regulation of FGF-23 in normal and hyp-mice. (A) Serum FGF-23 levels, measured by an assay specific for the intact molecule, was profoundly elevated in the hyp-mice, when compared to normal mice. (B) Consistent with this observation, real-time PCR measurements documented that Fgf-23 mRNA was likewise substantially elevated in the hyp-mouse bone samples. (C) Assessment of FGF-23 protein in the bone samples revealed a significant increase in intact FGF-23, but a significant decrease in the C-terminal FGF-23 fragments, evidence for impaired degradation. (D) Real-time PCR measurements of Bmp1 mRNA in bone samples from normal and hyp-mice revealed no difference in expression. However, assessment of BMP1 protein in these samples by Western blots documented that the pro-BMP1 protein was significantly increased and the active BMP1 significantly decreased in the hyp-mouse bone samples, consistent with impaired 7B2•PC2 cleavage of the pro-BMP1, as observed in the in vitro studies. (E) Real-time PCR measurements of Dmp1 mRNA in bone samples from normal and hyp-mice similarly revealed no difference in expression. However, consistent with decreased active BMP1 cleavage of DMP1, the bone samples from hyp-mice displayed a significant reduction in the N- and C-terminal DMP1 fragments and, as a result, significantly increased amounts of the full-length DMP1.

Figure 5.

Effects of D6R treatment on regulation of FGF-23 in normal and hyp-mice. (A) Real-time PCR measurements revealed a significant decrease in Sgne1 (7B2) mRNA in the bone from saline-treated hyp-mice. With D6R treatment of the hyp-mice for 5 weeks, a significant twofold increase in Sgne1 mRNA was realized, reaching levels no different than those in normal mice. Assessment of 7B2 protein by Western blots likewise documented a significant decrease in the saline-treated hyp-mice. In accord with the D6R-mediated enhancement of Sgne1 mRNA, the active protein increased significantly, again reaching a level comparable to those in the normal mice. (B) Real-time PCR measurements revealed that D6R treatment had no effect on Bmp1 mRNA in the bones of normal and hyp-mice. However, in response to treatment, the mutant mice normalized expression of the BMP1 active protein in bone samples, as evidenced on Western blots. Thus, although saline treated hyp-mice had significantly elevated pro-BMP1 and decreased active BMP1 in the bone samples, D6R treatment normalized the pro-BMP1 content and significantly increased the active BMP1 in hyp-mouse bone to levels no different than that in saline-treated mice. (C) Real-time PCR measurements revealed that D6R treatment had no effect on Dmp1 mRNA in the bones of normal and hyp-mice. However, D6R-treated mutant mice significantly increased the C-terminal DMP1 fragments to levels within the normal range, as evidenced on Western blots, reflecting increased proteolysis of the intact DMP1. The intact DMP1 (94 kDa) is not shown on the Western blots, because no bands were evident, despite loading substantial amounts of protein, due to efficient proteolysis, consistent with previous observations.37, 71 (D) Real-time PCR measurements documented that Fgf-23 mRNA was substantially elevated in the bone samples from saline-treated hyp-mouse bone samples, compared to that in saline-treated normal mice. However, D6R treatment of hyp-mice remarkably decreased the Fgf-23 mRNA to values no different than those documented in the saline- and D6R-treated normal mice.

Effects of Normalizing 7B2 and Enhancing 7B2•PC2 Activity on the HYP Phenotype

In subsequent studies, we treated hyp-mice with hexa-D-arginine amide (D6R) to determine if therapeutic enhancement of bone 7B2 production and 7B2•PC2 activity normalized the HYP phenotype. D6R was chosen because: (1) polyarginines are the only known stimulant of PC2 activity;49 (2) of the frequent coordinate regulation of 7B2 and PC250; and (3) preliminary studies documented that overnight incubation of TMob cells with D6R (50 µM) significantly increased Sgne1 (7B2) mRNA (1.0 ± 0.2 versus 2.8 ± 0.6 relative expression; p < 0.01).

Treatment of normal and hyp-mice for 5 weeks with either vehicle (saline) or D6R (1.5 µmol/g/day, i.p.) significantly increased the Sgne1 (7B2) mRNA and 7B2 protein to levels no different than those in normal mice (Fig. 5A). These observations suggest that D6R treatment, by normalizing the 7B2 protein content, increased the 7B2•PC2 enzyme activity in hyp-mouse bone. Indeed, further studies revealed that the 7B2•PC2-dependent intermediate steps in FGF-23 production, including osteoblast production of active BMP1 (Fig. 5B) and proteolytic degradation of DMP1 to its 57-kDa C-terminal product (Fig. 5C) were normalized. Consequently, D6R treatment decreased Fgf-23 mRNA expression to levels no different than those in normal mice (Fig. 5D).

Subsequent evaluation of bone from D6R-treated hyp-mice revealed restoration of normal bone length, as well as bone modeling and mineralization. As shown in Fig. 6A, saline-treated hyp-mice had shortened femurs, characteristic of the HYP phenotype. However, D6R treatment resulted in lengthening of the femurs from hyp-mice, while having no apparent effect on normal femurs. Indeed, measurement of femur length in normal and hyp-mice documented not only a significant shortening in the saline-treated mutants, but a significant increase in the D6R-treated hyp-mice to values approaching those in normal mice (Fig. 6A).

Figure 6.

Effects of D6R treatment on the HYP bone phenotype. (A) A representative radiograph of femurs in the saline and D6R-treated mice reveals that D6R treatment lengthens the characteristically shortened femur in hyp-mice to a length no different than that in normal mice, an observation confirmed by quantified data shown on the right. (B) Representative µCT images of the femurs from normal and hyp-mice treated with saline (upper panel) or D6R (lower panel) are shown with the whole-mount view on the left and sagittal sections on the right. The bone from saline-treated normal mice displays the classical rachitic features of rickets, porous bone, wide growth plates, and a large diaphysis. Treatment with D6R, however, restored normal bone modeling and calcification, resulting in normal bone architecture. (C) Representative µCT images of femur midshaft sections from saline (upper panel) and D6R-treated (lower panel) normal and hyp-mice. Bones from the saline-treated hyp-mice was porous and had an apparent reduced bone volume and enlarged cortical diameter, abnormalities normalized by D6R treatment, as confirmed by quantified data shown on the right. (D) Goldner-stained sections of cortical bone reveal at high magnification an increase in unmineralized osteoid (red-brown colored) in the saline-treated hyp-mouse bone, compared with that in saline- and D6R-treated normal mice. However, D6R-treatment of hyp-mice resulted in apparently normal histomorphology, as confirmed by quantitative assessment of osteoid area (OA/TA) and mineralized area (MA/TA), shown on the right. (E) Calcein green and Alizarin complexone dye double-labeled bone specimens, viewed under fluorescent light, show abnormal mineralization in the bone sections from saline-treated hyp-mice, as evidenced by smudged fluorescent labels, which are in marked contrast to the distinct dual labels evident in normal mice. However, D6R treatment of hyp-mice resulted in the presence of distinct dual fluorescent labels, set apart a similar distance as in normal mice. As shown on the right, these observations were confirmed by quantitative assessment of the mineral apposition rate, which was normal in the bone sections from D6R-treated hyp-mice.

Further examination of the femurs by µCT revealed that saline-treated hyp-mice had poor mineralization of bone, associated with abnormal bone modeling. Whole-mount and sagittal bone sections from saline-treated hyp-mice displayed the classical features of rickets, including reduced length, increased width, porous bone, wider growth plates, and an enlarged diaphysis (Fig. 6B). Treatment with D6R restored bone modeling and calcification, reducing the width of the bones, decreasing porosity, and restoring normally sized growth plates and diaphyses. Similarly, µCT images of femur midshaft sections revealed increased porosity, an apparent reduced bone volume, and a commensurately enlarged cortical diameter. Again, D6R treatment showed restoration of normal bone architecture (Fig. 6C). The changes observed in µCT images of femur midshaft sections were confirmed by quantified bone volumetric data. Bone from the D6R-treated hyp-mice displayed a significant increase in bone volume, achieving values no different from those in normal mice (Fig. 6C).

These observations were supported by analysis of Goldner-stained bone sections obtained from saline- and D6R-treated mice (Fig. 6D). Compared to similarly treated normal mice, saline-treated hyp-mice had abundant brown-staining osteoid, distributed in widened seams over the bone surface and within pockets found in the mineralized trabecular bone. D6R treatment of hyp mice abolished the excess osteoid and quantitative histomorphology revealed that the osteoid in the D6R-treated hyp-mice significantly declined to levels no different than those in normal mice. Reciprocally, the mineralized area also normalized (Fig. 6E). Assessment of the bone mineral apposition rate confirmed the presence of normal mineralization (Fig. 6F). Whereas saline-treated normal mice displayed evidence of crisp double fluorescent bone labels, indicative of normal mineralization, fluorescent labeling in the long bones of hyp-mice was diffuse and smudged, indicative of abnormal mineralization. D6R treatment had no effect on the crisp double labels in normal mice, while remarkably altering mineralization dynamics in hyp-mice, inducing distinct double labels in the bone sections, consistent with normal mineralization. Quantitative histomorphology revealed that a profoundly decreased mineral apposition rate in saline-treated hyp-mice increased to normal levels upon treatment with D6R (Fig. 6G).

We further examined D6R-treated hyp-mice to determine if therapy also normalized the HYP biochemical abnormalities. Administration of D6R to hyp-mice increased the serum Pi asymptotically from a baseline of 3.2 ± 0.2 mg/dL to a maximum of 6.6 ± 0.4 mg/dL (p < 0.001) (Fig. 7A). A significant increase in the serum Pi concentration was evident after only 3 days of treatment, and the serum Pi increased progressively to a peak at 21 days of treatment. Perhaps more importantly, whereas the serum Pi levels in the D6R-treated hyp-mice from days 0 to 18 were significantly less than those in the saline- and D6R-treated normal mice, values from 21 to 35 days of treatment were significantly greater than those at 18 days and no different than those in the normal mice (Fig. 7A). Normalization of the serum Pi occurred due to an increase of renal tubule Npt2a mRNA and NPT2a protein, to levels comparable to those in saline- or D6R-treated normal mice (Fig. 7B).

Figure 7.

Effects of D6R treatment on phosphate, vitamin D, and FGF-23 homeostasis in hyp-mice. (A) The 5-week D6R treatment course significantly increased the serum phosphorus concentration, compared to baseline, from day 3 through day 35. The increase in the serum phosphorus concentration in the D6R-treated hyp-mice progressed asymptotically, with values from days 3 to 18 significantly lower than those in the saline and D6R-treated normal mice. However, at the asymptotic maximum from days 21 to 35 of treatment, the serum phosphorus level was significantly greater than those from days 3 to 18, but more importantly no different than those in the saline- and D6R-treated normal mice. Throughout the treatment period the saline-treated hyp-mice maintained a serum phosphorus concentration significantly less than the D6R-treated hyp-mice and the saline- and D6R-treated normal mice. (B) The normalization of the serum phosphorus concentration in the D6R-treated hyp-mice was accompanied by a significant increase in the real-time measurements of renal Npt2a mRNA expression at 35 days, to values no different than those in saline- and D6R-treated normal mice. Similarly, the renal NPT2a protein content in the D6R-treated hyp-mice, assessed by Western blots, increased significantly to values no different than in saline- and D6R-treated normal mice. (C) Compared to saline-treated hyp-mice, the D6R-treated mutant mice displayed a significant decrease of the renal Cyp27b1 (25(OH)D-1α-hydroxylase) mRNA expression to values no different than those in saline- and D6R-treated normal mice. The unchanging expression of the 25(OH)D-1α-hydroxylase protein and enzyme activity in the D6R-treated hyp-mice indicated that treatment had corrected the abnormal translational regulation of enzyme activity in the mutant mice. (D) Serum FGF-23 levels, measured by an assay specific for the intact molecule and a C-terminal specific assay, was profoundly elevated in the saline-treated hyp-mice. In concert with the normalization of Fgf-23 mRNA (see Fig. 5E) and enhanced FGF-23 degradation, D6R treatment of hyp-mice significantly decreased the circulating FGF-23 levels, as measured by both assays. Comparing the data from the two assays, there is a 30% decrease, when using the measurement of intact FGF-23 and only a 24% decrease, when using the C-terminal assay, a difference consistent with an inordinate increase in the circulating C-terminal fragment likely due to a normalization of FGF-23 degradation.

Additionally, in response to D6R treatment, the increased renal Cyp27b1 (25(OH)D-1α-hydroxylase) mRNA expression seen in hyp-mice decreased to values similar to those in saline- and D6R-treated normal mice (Fig. 7C). The unchanged expression of 25(OH)D-1α-hydroxylase protein and activity in D6R-treated hyp-mice (Fig. 7C) suggested that treatment had corrected the abnormal translational regulation of enzyme activity in the mutant mice.

However, as shown in Fig. 7E, although the serum FGF-23 concentration in D6R-treated hyp-mice decreased significantly, when measured by the intact and carboxy-terminal specific assays the level remained substantially increased. The elevated serum FGF-23 level persisted, despite normalization of bone Fgf-23 mRNA (Fig. 5D), complete resolution of the HYP phenotype, and no end organ evidence of increased Fgf-23 bioactivity. Nevertheless, because the magnitude of the decrement was less, when examined using the carboxy-terminal specific assay, it is likely that the D6R treatment had increased hormone degradation, and treated hyp-mice had a relative increase in the circulating levels of the FGF-23 carboxy-terminal fragments.

Discussion

Despite apparent progress in understanding the pathophysiological basis for XLH, few advances have been made in defining an effective treatment for the disease. This failure is related to a unique block to treatments based on genetic complementation in this disorder. Classic complementation therapy has been precluded in this single-gene (PHEX/Phex) defect disease by the inability to rescue the phenotype by overexpression of PHEX24–26 in hyp-mice and the failure to define a PHEX substrate.21 However, discovery that a major PHEX-dependent abnormality in XLH is increased circulating FGF-23, which is strongly associated with the genesis of the HYP phenotype, appeared to offer a realistic alternative strategy for treatment via blockade of FGF-23 effects. Unfortunately, this approach has been severely limited by the incomplete response of the disease phenotype to antibody neutralization.27, 28

Alternative approaches to modifying FGF-23 effects for a therapeutic purpose requires better understanding the mechanisms underlying the decreased degradation and increased production of this phosphatonin in health and in XLH. In the current studies, we used a variety of traditional biochemical and molecular biological techniques to explore the regulation of FGF-23 degradation and production both in vitro and in vivo. We initially demonstrated that general inhibition of proprotein convertase activity in normal mice increased circulating levels of FGF-23, decreased serum phosphorus, and induced posttranscriptional inhibition of 25(OH)D-1α-hydroxylase activity, changes that recapitulate the cardinal biochemical features of the HYP phenotype. Upon ascertaining that PC2 was a likely candidate convertase contributing to regulating FGF-23, we investigated whether this enzyme can alter FGF-23 degradation and production in vitro.

Proprotein convertases are responsible for the tissue-specific processing of multiple polypeptide precursors in a wide variety of tissues and cell lines.38, 44, 51, 52 However, PC2 differs from other proprotein convertases in its specific requirement for a chaperone protein, 7B2. Numerous studies have shown that PC2 maturation and enzyme activity are uniquely regulated by 7B2, and that PC2 expressed in the absence of 7B2 is incapable of autoactivation or substrate cleavage.46, 53–57 In accord with these observations, we showed that transfection of TMob cells with Sgne1 (7B2) and Pcsk2 (PC2) results in FGF-23 cleavage, whereas expression of Sgne1 or Pcsk2 alone has no effect. Moreover, FGF-23 degradation is blocked in TMob cells by Sgne1 RNA-induced knockdown of Sgne1 expression. These findings are consistent with the known presence of a convertase cleavage site in FGF-23 between amino acids 179 and 180 in the Arg-Arg-His-Thr-Arg motif, which in ADHR limits FGF-23 proteolysis and increases serum FGF-23.8–10 Although many previous studies have shown that furin can mediate cleavage at this site29, 58, 59 and PC2 is capable of cleaving either at the Arg-Arg site, or at single arginines in the presence of an upstream arginine,60 our investigations indicate that PC2 may play a larger role than furin in this cleavage event in bone.

Subsequent investigations revealed that 7B2•PC2 activity regulates not only FGF-23 degradation, but FGF-23 production as well. Thus, transfection of TMob cells with a Sgne1 (7B2) expression vector significantly decreased Fgf-23 mRNA, whereas an increase in Fgf-23 mRNA was detected upon Sgne1 (7B2) RNAi inhibition of mRNA and protein expression. Further experiments linked the effects of decreased 7B2•PC2 activity on FGF-23 production to reduced proteolysis of proBMP1, which resulted in limited cleavage of DMP1 to its 37-kDa N- and 57-kDa C-terminal fragments. The apparent impact of DMP1 on FGF-23 supports an important role for DMP1 proteolysis in the regulation of Fgf-23 mRNA expression. However, although the unique effects of BMP1 on DMP1 proteolysis were known,46 the apparent role of PC2 on proBMP1 cleavage was somewhat unexpected, because Golgi-localized furin represents the dominant convertase responsible for this cleavage event in the only cell type tested thus far, HT1080 cells.46 However, the Arg-Ser-Arg-Arg site cleaved within proBMP1 is a PC2 recognition cleavage site,60 providing justification for further work to establish the contribution of PC2 to proBMP1 cleavage in bone cells and tissue.

It is important to note that BMP1 is not the only enzyme that cleaves DMP1. Recent studies50 have documented that matrix metalloproteinase-2 (MMP2), a membrane-bound enzyme, also cleaves the intact DMP1. However, the cleavage products include a 42-kDa carboxy-terminal fragment, which appears to have biological effects in dental pulp. The absence of the DMP1 42-kDa carboxy-terminal fragment in the normal and hyp-mouse bone, or the TMob cells, indicates that the 7B2-PC2 mediated cleavage of DMP1 is dependent on generation of active BMP1.

Although these data clearly establish that decreased 7B2•PC2 activity is associated with reduced FGF-23 degradation and increased hormone production in vitro, the role that such altered enzyme function might play in XLH remained uncertain. Therefore, we examined whether defective expression of either 7B2 or PC2 occurred in hyp-mice. Bone obtained from the mutant mice exhibited significantly decreased expression of both Sgne1 (7B2) mRNA and 7B2 protein. These decreased levels of 7B2 limit cleavage not only of FGF-23, but of proPC2 as well, as evidenced by the presence of an increased ratio of proPC2 to active PC2. These observations are consistent with previous reports in the Sgne1 null mouse45 and in cell culture,48, 55 and support the concept that reduction in 7B2 levels results in decreased bone PC2 activity in XLH.

The possibility that a primary defect in hyp-mice is reduced 7B2 was confirmed by further studies that revealed expected downstream effects of decreased 7B2•PC2 activity. As previously found,22, 23 hyp-mice exhibit significantly increased levels of serum FGF-23, as a result of both decreased FGF-23 degradation and increased FGF-23 production. Consistent with our in vitro studies, increased FGF-23 production in hyp-mouse bone was associated with decreased BMP1-mediated degradation of DMP1 and decreased genesis of the C-terminal DMP1 fragment. Although the increase in Fgf-23 mRNA may not result directly from the decreased concentrations of the DMP1 carboxy-terminal fragment, our in vitro studies, and the recent reports that establish transgenic overexpression of the C-terminal DMP1 fragment is essential to rescue the Dmp1 null phenotype and normalize serum FGF-23,36–38 support DMP1 proteolysis-mediated regulation of FGF-23 production in the hyp-mouse. In summary, these results establish that diminished 7B2 production in bone represents a critical step in the pathogenesis of the HYP phenotype (Supplementary Fig. S3), although the mechanism(s) by which the Phex mutation causes downregulation of 7B2 expression in hyp-mice remains unknown.

Although the well-known functional link between 7B2 and PC2 implies that their expression is coordinately regulated, the data obtained in the hyp-mouse model support the idea of discordant regulation. Indeed, such discordant regulation has been previously reported. Thus, while stimulation of P19 neuronal cells via a protein kinase C-mediated pathway coordinately increases expression of both 7B2 and PC2, protein kinase A-mediated stimulation increases expression of PC2 alone.60 Moreover, a growing body of evidence suggests 7B2 expression frequently controls PC2 activity in hormonal peptide production.61 The molecular details of the control of 7B2 expression are only now beginning to emerge, with recent studies pointing to promoter polymorphisms which clearly control expression57, 62; ie, a 5′ regulatory region in Sgne1 (7B2) mRNA, which acts to repress expression62 and epigenetic control by differential methylation of the Sgne1 gene.63–65 The relative contributions of these various regulatory mechanisms to the control of 7B2 expression in bone is not yet known.

Although our in vivo observations support the possibility that 7B2-dependent, PC2-mediated alterations in FGF-23 degradation and production are operative in the hyp-mouse osteoblast, the singular role of this abnormality in the genesis of the HYP phenotype was still unclear. To explore this issue further, we sought to pharmacologically normalize PC2 activity in order to increase FGF-23 degradation and decrease production. The effects observed in D6R-treated hyp-mice were indeed remarkable. As anticipated, treatment resulted in a significant increase in the bone Sgne1 (7B2) mRNA and 7B2 protein and no doubt concordant enhancement of 7B2•PC2 enzyme, which resulted in apparent normalization of the HYP phenotype. Indeed, during the 5-week period of treatment, serum phosphorus levels increased progressively to values maintained from days 21 to 35 that were no different than those of normal mice. These changes were clearly secondary to a significant increase in the renal Npt2a mRNA and NPT2a protein. Likewise, administration of D6R corrected the abnormal translational regulation of renal 25-hydroxyvitamin D-1α-hydroxylase activity, characteristic of the hyp-mouse.

Further, D6R treatment not only normalized the biochemical abnormalities, but had profound effects on bone architecture, remodeling, and mineralization. Thus, bone length was returned to normal in the hyp-mice, as was bone modeling and mineralization. These changes resulted in long bones with normal width and size of the growth plates and diaphyses. Moreover, restoration of mineralization dynamics included establishing a normal mineral apposition rate and eliminating all evidence of excess unmineralized osteoid. Complete resolution of the rickets and osteomalacia in response to D6R treatment is in marked contrast to the effects of alternative therapeutic regimens. Previous treatment strategies for XLH in affected humans and mice have included vitamin D and phosphorus,66 calcitriol and phosphorus,67, 68 antibody neutralization of Fgf-23,28 and PHEX overexpression,24–26 all of which invariably remarkably improve the biochemical phenotype, but uniformly fail to heal the bone disease, particularly the osteomalacia. Thus, treatment with D6R influences bone mineralization in an unprecedented fashion.

The effects noted in the preceding paragraphs were those anticipated with the D6R-mediated increase in bone Sgne1 mRNA and protein, and consequent enhanced 7B2•PC2 enzyme activity. Although the molecular mechanism by which D6R increases Sgne1 message levels in bone cells remains unknown, the expected result of such enhanced activity is restoration of normal FGF-23 production and degradation, and accordingly reduction of the stimulus for the abnormal biochemistries and bone morphology and histology present in hyp-mice. Indeed, in response to D6R treatment we observed decreased transcription of Fgf-23 mRNA, along with the predicted enhanced BMP1 activation and elevated proteolytic degradation of DMP1. However, the serum FGF-23 level in the D6R-treated hyp-mice remained elevated when measured using the intact and carboxy-terminal immunoassays. Nevertheless, comparison of the measurements by these techniques revealed a greater decrement when assessed using the intact immunoassay, suggesting that degradation of the intact FGF-23 was enhanced and perhaps normalized.

The explanation for this incongruous elevation of the serum FGF-23 concentration is not immediately apparent. Measurement of serum FGF-23 at multiple dilutions in D6R-treated hyp-mice produced results that diluted parallel to the standard curve, eliminating co-measurement of an unrelated factor. It is also unlikely that the bioactivity of the circulating FGF-23 is decreased by a limited interaction of the hormone with its receptor, FGF1R, due to either a decrease in the renal klotho protein, a key component of the binary complex that creates FGF1R,69 or competitive inhibition of the intact FGF-23 binding to its receptor by the C-terminal FGF-23, consistent with recently reported findings.70 It is possible that structural differences in the circulating FGF-23 in treated hyp-mice may influence measurement of the intact molecule, consistent with the extraosseous clearance of intact FGF-23, about which little is known. No data are available that indicate such degradation of circulating FGF-23 generates the classic N- and C-terminal fragments. With the absence of any evidence of increased bioactivity at the kidney or bone, it seems plausible that extraosseous degradation of remarkably elevated serum levels of intact FGF-23 may generate abundant amounts of a bioinactive FGF-23 fragment, which includes the antigenic epitope(s) recognized by the antibodies used in the ELISA measurement. Since the antigenic epitopes are at the N-terminal and C-terminal cleavage sites, the bioinactive fragment may result from cleavage of the intact FGF-23 at site(s) distal to the normal N- and C-terminal cleavage site, rendering the molecule bioinactive but preserving the antigenic epitopes. Additional studies, outside the scope of the present investigation, will be necessary to establish with certainty if the elevated serum FGF-23 level, in association with normal bioactivity at kidney and bone, represents interference of hormone binding to its receptor, circulation of a bioinactive fragment of FGF-23, detected by the ELISA assay, or another event.

Regardless, our studies indicate that the loss-of-function Phex mutation in hyp-mice results in decreased osseous 7B2 production, a protein essential for manifestation of PC2 activity. The loss of 7B2 results in diminished PC2 activity and significantly limits cleavage of FGF-23 and proBMP1 and, indirectly, of DMP1. The physiological consequences that ultimately result from the 7B2 defect are increased levels of circulating FGF-23 and consequent renal phosphate wasting, abnormal transcriptional regulation of renal 25-hydroxyvitamin D-1α-hydroxylase activity, and rickets/osteomalacia. Most importantly, we found that the polyarginine D6R apparently restores the activity of PC2, most likely by increasing 7B2 production. D6R thus normalizes the HYP phenotype, correcting phosphate and vitamin D homeostasis, as well as bone modeling and mineralization. Whereas much work remains to establish the cellular and molecular mechanisms for PHEX-7B2 interactions, the findings presented here provide novel insight into the biosynthetic mechanisms of FGF-23 synthesis, and, most importantly, create a biochemical basis for a fully curative drug treatment regimen for XLH.

Disclosures

Drs. Drezner and Yuan have filed a use patent for Hexa-D-Arginine, US Patent Application #13/272809, Drezner et al (patent pending). The authors have no other conflicts of interest.

Acknowledgements

This work was funded by NIH grants (R01-AR27032, R01-SK65830, and 1UL1RR025011 to MKD; R01-DE018486 to JQF; AR54753 to RDB; and DK049703 to IL) and a Veterans Administration grant to RD Blank (Merit Award). The work reported in this article was conducted in the VAMC Geriatrics Research, Education, and Clinical Center, Madison, WI, USA.

Authors' roles: Study design: MKD, BY, IL, and RDB. Study conduct: BY, SB and YL. Data collection: BY, SB, and YL. Data analysis: MKD, BY, IL, JQF, and RDB. Drafting of manuscript: MKD and BY. Revising of manuscript: MKD, BY, IL, JQF, and RDB. Obtained funding: MKD, JQF, RDB, and IL.

Ancillary