• Journal of Periodontal and Implant Science
• /
• v.26 no.1
• /
• pp.1-26
• /
• 1996

This study was performed to estimate the effects of cultured bone cell inoculated on porous type hydroxyaptite for the regeneration of the artificial alveolar bone defect. In this experiment 3 beagle dogs were used, and each of them were divided into right and left mandible. Every surgical intervention were performed under the general anesthesia by using with intravenous injection of Pentobarbital sodium(30mg/Kg). To reduce the gingival bleeding during surgery, operative site was injected with Lidocaine hydrochloride(l:80,000 Epinephrine) as local anesthesia. After surgery experimental animal were feeded with soft dietl Mighty dog, Frisies Co., U.S.A.) for 1 weeks to avoid irritaion to soft tissue by food. 2 months before surgery both side of mandibular 1st premolar were extracted and bone chips from mandibular body were obtained from all animals. Bone cells were cultured from bone chips obtained from mandible with Dulbecco's Modified Essential Medium contained with 10% Fetal Bovine Serum under the conventional conditions. Porous type hydroxyapatite were immerse into the high concentrated cell suspension solution, and put 4 hours for attachin the cells on the surface of hydroxyapatite. Graft material were inserted on the artificial bone defect after 3 days of culture. Before insertion of cellinoculated graft material, scanning electronic microscopic observation were performed to confirm the attachment and spreading of cell on the hydroxyapatite surface. 3 artificial bone defects were made with bone trephine drill on the both side of mandible of the experimental animal. First defect was designed without insertion of graft material as negative control, second was filled with porous replamineform hydroxyapatite inoculated with cultured bone marrow cells as expermiental site, and third was filled with graft materials only as positive control. The size of every artificial bone defect was 3mm in diameter and 3mm in depth. After the every surgical intervention of animals, oral hygiene program were performed with 1.0% chlorhexidine digluconate. All of the animals were sacrificed at 2, 4, 6 weeks after surgery. For obtaining histological section, tissus were fixed in 10% Buffered formalin and decalcified with Planko - Rycho Solution for 72hr. Tissue embeding was performed in paraffin and cut parallel to the surface of mandibular body. Section in 8um thickness of tissue was done and stained with Hematoxylin - Eosin. All the specimens were observed under the light microscopy. The following results were obtained : 1. In the case of control site which has no graft material, less inflammatory cell infiltration and rapid new bone forming tendency were revealed compared with experimental groups. But bone surface were observed depression pattern on defect area because of soft tissue invasion into the artificial bone defect during the experimental period. 2. In the porous hydroxyapatite only group, inflammatory cell infiltration was prominet and dense connective tissue were encapsulated around grafted materials. osteoblastic activity in the early stage after surgery was low to compared with grafted with bone cells. 3. In the case of porous hydroxyapatite inoculated with bone cell, less inflammatory cell infiltration and rapid new bone formation activity was revealed than hydroxyapatite only group. Active new bone formation were observed in the early stage of control group. 4. The origin of new bone forming was revealed not from the center of defected area but from the surface of preexisting bony wall on every specimen. 5. In this experiment, osteoclastic cell was not found around grafted materials, and fibrovascular invasion into regions with no noticeable foreign body reaction. Conclusively, the cultured bone cell inoculated onto the porous hydroxyapatite may have an important role of regeneration of artificial bone defects of alveolar bone.

• Journal of Veterinary Clinics
• /
• v.26 no.2
• /
• pp.144-149
• /
• 2009

Chondrocytes and synovial fluid derived markers are used to monitor for osteoarthritis(OA). Specific inhibitors, known as tissue inhibitors of metalloproteinases(TIMP), regulate the proteolytic activity of matrix metalloproteinases(MMP). This study investigated whether MMP and TIMP levels were altered in synovial fluid and cartilage following the experimental induction of OA in canines. Twenty mature beagle dogs underwent a unilateral surgical transection of the cranial cruciate ligament and the medial collateral ligament as well as a medial meniscectomy. Matrix metalloproteinase-2 and MMP-9 levels were assayed using Western blot and TIMP-2 levels were measured with enzyme-linked immunosorbent assays four weeks after OA induction. Increased MMP-2 expression was observed in chondrocytes isolated from cartilage following OA induction, but MMP-9 expression decreased. Matrix metalloproteinase-2 and MMP-9 levels in synovial fluid from the OA induced joint significantly increased compared to those of the sham group. Tissue inhibitors of metalloproteinase-2 concentrations were higher in chondrocytes from the OA cartilage, yet TIMP-2 remained lower in the synovial fluid of OA. This suggests the elevated release of MMP-9 over MMP-2 into the synovial fluid following the cartilage degradation-related death of chondrocytes after OA. Osteoarthritis can be further deteriorated by increased MMP activity in the synovial fluid because TIMP-2 exist low concentration into the extracellular matrix. As a result, MMP activity, particularly MMP-9 activity, can be useful as a biomarker in diagnosing and monitoring the early stages of canine OA.

• Journal of Veterinary Clinics
• /
• v.27 no.5
• /
• pp.546-552
• /
• 2010

Previous studies could not offer available guideline to decide size of balloon and grade of injury before induction of spinal cord injury (SCI) because grade of SCI was assessed after inserting a catheter and each experimental animal were different in body size and weight as well as in species. This study was performed to provide guideline for standardized SCI model. Eight healthy adult beagle dogs that had 8 mm of spinal canal height were assigned to four groups according to the diameter of balloon and compression time: 4 mm/3hrs, 4 mm/6hrs, 4 mm/12hrs and 6 mm/3hrs group. Radiography was performed to standardize between experimental animal and balloon before selecting balloon diameter to induce SCI. Behaviors outcomes, somatosensory evoked potentials (SEPs), magnetic resonance imaging (MRI) and histopathological examination were evaluated. Behaviors outcomes and SEPs were not available to assess grade of SCI and those only indicate SCI. The damaged area was revealed clear hyperintensity on STIR image and T2WI after induction of SCI. The hyperintense area on MRI was cranially and caudally expanded with increasing of the diameter of balloon or the compression time. Well corresponded to expanding of hyperintense area on MRI, the damaged region and the numbers of caspase-3 and PARP immunoreactive cells were increased on histopathological findings. Therefore, these results will be considered fundamental data to induce standardized SCI model in experimental animal that has various weight and size.

• Journal of Preventive Medicine and Public Health
• /
• v.28 no.4 s.51
• /
• pp.863-873
• /
• 1995

This report describes a preperation and characterization of canine blood lead(Pb) standard reference material(SRM). Three adult beagle dogs(A, B, and C)were orally dosed with gelatin capsules containing $Pb(NO_3)_2$, equivalent to $10\sim80mg$ Pb/kg body weight. Blood was drawn 24 hours after the dose from the cephalic vein into lead free 500ml Pyrex beaker in which EDTA.K was contained as an anticoagulant. The amount of lead given to individual dog was varied arbitrarily. Three month later, 3 canine animals were orally dosed with lead secondarily to make mixed SRM(D1) which was mixed different concentrations of lead in bloods with A1, B1, and C1 in vitro. The SRMs for A, B, C, A1, B1, C1, and D1 were distributed 2ml each into more than 300 lead free bottles, and were stored in refregerator at $4^{\circ}C$. The amount of lead in canine whole blood samples were determined using a Varian 30A atomic absorption spectrophotometer(AAS) with a model GTA-96 graphite tube atomizer with D2 background correction and a Hitachi Z-8100 AAS with Zeeman background correction. The sensitivity and detection limits for lead determination of Varian 30A were $0.46{\mu}g/L,\;0.34{\mu}g/L,\;and\;0.56{\mu}g/L,\;0.14{\mu}g/L$ of Hitachi Z-8100, respectively. Day to day variations in determination of blood lead concentration in a certain sample were $31.11{\pm}1.36{\mu}g/100ml$ by Varian 30A, and $33.08{\pm}0.82{\mu}g/100ml$ by Hitachi Z-8100, showing the difference of 3% between the two results. At the blood lead concentrations of $56.31{\pm}1.98{\mu}g/100ml(A),\;40.89{\pm}0.80{\mu}g/100ml(B),\;59.01{\pm}1.38{\mu}g/100ml(C)$, the precisions of replicated measurements by AAS were 3.52%, 1.96%, and 2.34%, respectively. Coefficient variation(CV) of SRMs(A, B, and C) within a standard sample were ranged from 0.92% to 7.50%, and those between 5 standard samples were 1.21%, 2.64%, and 1.11%, respectively, showing inter-vial variation of $1{\mu}g/100ml$. Lead levels in SRMs during one month storage were unchanged. The overall recoveries were $89.6\sim100.4%,\;91.6\sim101.9%,\;90.3\sim100.0%$ for A, B, and C SRMs, means were $56.46{\pm}2.69{\mu}g/100ml,\;39.35{\pm}1.89{\mu}g/100ml,\;57.40{\pm}2.31{\mu}g/100ml$, and measurement ranges were$52.88{\pm}59.26{\mu}g/100ml,\;37.47{\pm}41.68{\mu}g/100ml,\;54.80{\pm}60.69{\mu}g/100ml$, respectively. Those results were laid within confidence limits values. The lead concentrations in the mixed sample(D1) stored over one month period were ranged from $32.76{\mu}g/100ml\;to\;33.54{\mu}g/100ml$, with CV ranging from 1.2% to 2.7%. The results were similiar to each of single samples(A1, B1, and C1) in respect of homogeneity and stability. Results of the mixed blood sample analysed after 1 month storage at $4^{\circ}C$ by four other laboratories(L1, L2, L3, L4) were similar with those of our laboratory($L5;31.18{\pm}0.24{\mu}g/100ml$, acceptable range by $CDC;25.18\sim37.18{\mu}g/100ml$), showing the concentrations of $25.91{\pm}1.19{\mu}g/100ml(L1),\;34.16{\pm}0.22{\mu}g/100ml(L2),\;35.68{\pm}0.85{\mu}g/100ml(L3),\;30.95{\pm}0.46{\mu}g/100ml(L4)$ in a each samples.