Osseointegration of novel silver-doped hydroxyapatite
coated and acid-etched titanium implants in an ovine
model
Dasun Abeygoonawardana
A thesis in fulfilment of the requirements for the degree of
Master of Science
Prince of Wales Clinical School
Faculty of Medicine
March 2017
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Date Abstract
Despite advances in technology and surgical procedures, periprosthetic infection of orthopaedic implants remains a common and costly cause of implant failure and revision. Novel materials and coatings have been developed in an effort to improve implant resistance to the onset of infection, including those utilising the antimicrobial properties of silver ions. The aims of this study were to evaluate the osseointegration of a novel silver-doped hydroxyapatite coating and a second acid-etching process, applied to a titanium implant substrate implanted using a well-established ovine model. The subsequent results from the silver-doped coating could be compared to conventional hydroxyapatite coatings, to evaluate the effect of silver ions upon potential bone ongrowth. In this study, the silver HA coated implants demonstrated significantly higher shear stresses of mechanical pushout when compared to the acid etched implants after 4 weeks and 12 weeks in situ. Similarly, the bone-implant contact percentage was significantly higher for the silver HA coated implants indicating greater osseointegration at both timepoints. When compared to conventional HA coated implants in an identical ovine model, there was no significant difference observed in mechanical pushout or bone- implant contact of the silver HA coated implants. These results indicate that the novel silver-doped HA coating does not adversely affect the osseointegration of titanium implants. Therefore, this represents a viable solution for an antimicrobial implant coating which continues to facilitate effective osseointegration following implantation.
ii Table of Contents
List of Figures ...... v
List of Tables ...... vii
Acknowledgements ...... viii
Chapter 1. Introduction ...... 9
1.1 Infection and revision of orthopaedic implants ...... 9 1.2 Economic impact of prosthetic infection ...... 10 1.3 Mechanisms of prosthetic infection ...... 11 1.4 Antimicrobial properties of silver ions ...... 14 1.5 Use of silver in current implant technology ...... 15 Chapter 2. Method ...... 18
2.1 Study Design Summary ...... 18 2.2 Implant Manufacture ...... 19 2.3 Animal Preparation ...... 21 2.4 Cortical Site Implantation ...... 21 2.5 Cancellous Site Implantation ...... 23 2.6 Post-operative Recovery ...... 24 2.7 Harvest and Sample Preparation ...... 25 2.8 Mechanical Testing ...... 28 2.9 SEM Sample Preparation ...... 30 2.10 SEM Imaging...... 32 2.11 Histomorphometry ...... 33 2.12 Histology ...... 34 Chapter 3. Results ...... 35
3.1 SEM Coating Characterisation ...... 35 3.2 Surgery and Harvest ...... 37 3.3 Radiography ...... 38 3.4 Mechanical Testing ...... 43 3.5 SEM Imaging...... 48 3.6 Histomorphometry ...... 48 3.7 Histology Findings ...... 51
iii Chapter 4. Discussion ...... 55
4.2 Comparison of results with other ovine model studies ...... 57 4.3 Effect of surface topology upon bone ongrowth ...... 61 4.4 Current developments of silver in implants...... 68 4.4.1 Functionalised HA Coatings ...... 68 4.4.2 Silver-doped Strontium coatings...... 72 4.4.3. Agluna® material ...... 76 4.4.4 PorAg® coating ...... 80 4.5 Silver concentrations of current implants and coatings ...... 81 4.6 Ag HA compared to conventional HA ...... 83 4.7 Study Limitations and Future Studies ...... 87 Chapter 5. Conclusions ...... 90
References ...... 92
Appendix A Histomorphometric Results ...... 97
Results from W2602...... 98 Results from W2603...... 99 Results from W2604...... 100 Results from W2605...... 101
iv List of Figures
Figure 1 Three cortical implants in tibial diaphysis of animal W2603 showing implant flush with bone surface ...... 22 Figure 2 Implantation overview of ovine model showing four implantation scenarios in cancellous sites and line-to-line implantation in bicortical sites [54] ...... 23 Figure 3 Step drill used in surgery to provide a range of implantation scenarios within a single site ...... 24 Figure 4 Isolated femur and tibia (both left and right) from animal W2603 ...... 26 Figure 5 Isolated axial segment from tibial diaphysis containing cortical implant ...... 27 Figure 6 Sample W2602L4 following sectioning, showing medial half (W2604L4-M) ...... 28 Figure 7 Raw SEM image of Specimen W2604R5L at 80x magnification. Implant (blue arrow) is displayed as white, while bone (red arrow) is displayed as grey. Voids (circled) are represented as darker regions...... 32 Figure 8 SEM images of Specimen W2604R5L showing raw (top) and processed (below) versions. Green represents regions of bone contact, red represents bone voids. Total bone contact is 85.2%, as indicated in top left corner of processed image...... 33 Figure 9 SEM imaging of acid etched surface (Group 1) (x50 magnification). Texturing and evenly distributed ridges achieved through acid-etching process visible ...... 35 Figure 10 SEM imaging of Ag HA (Group 2) coating (x50 magnification). Unique surface of plasma-spray coating visible in the form of compact undulations and microstructures...... 35 Figure 11 SEM imaging of acid etched surface (Group 1) (x1000 magnification). Network of ridges, crevices and nanopits visible at this level of magnification...... 36 Figure 12 SEM imaging of Ag HA coating (x250 magnification). Small voids and porous regions visible between the plasma-sprayed structures of the Ag HA coating...... 36 Figure 13 Harvested tibia from W2605 showing visible cancellous (blue arrow) and cortical (red arrow) implantation sites. Not evidence of foreign body reaction or implant rejection surrounding implants in situ ...... 38 Figure 14 Left limb radiographs of animal W2602, AP(left) and lateral (right) views, showing good implant alignment at all sites ...... 39 Figure 15 Right limb radiographs of animal W2602, AP(left) and lateral (right) views, showing good implant alignment at all sites ...... 39 Figure 16 Left limb radiographs of animal W2603, AP(left) and lateral (right) views, showing good implant alignment at all sites ...... 40 Figure 17 Right limb radiographs of animal W2603, AP(left) and lateral (right) views, showing good implant alignment at all sites ...... 40 Figure 18 Left limb radiographs of animal W2604, AP(left) and lateral (right) views, showing good implant alignment at all sites ...... 41 Figure 19 Right limb radiographs of animal W2604, AP(left) and lateral (right) views, showing good implant alignment at all sites ...... 41 Figure 20 Left limb radiographs of animal W2605, AP(left) and lateral (right) views, showing good implant alignment at all sites ...... 42
v Figure 21 Right limb radiographs of animal W2605, AP(left) and lateral (right) views. Implant alignment was sufficient at all sites...... 42 Figure 22 Force-displacement curve output from custom Matlab script. Green line indicates stiffness (N/mm) taken from initial linear portion. Shaded blue region indicates integral area calculated for energy to failure (J). Peak load is the force value corresponding to junction between blue and white shaded regions...... 44 Figure 23 Mean shear stress of pushout at 4-week and 12-week timepoints for acid-etched and Ag HA implant groups. Error bars indicate standard deviation. Ag HA implants had significantly higher shear stresses at both timepoints...... 47 Figure 24 10x magnification of W2605L5L, showing Haversian systems (arrowed) and dense woven bone (circled) in proximity of Ag HA coating ...... 51 Figure 25 10x magnification of W2605R5M, showing rounded and enlarge osteoblasts layered upon newly formed bone (arrowed) at various sites ...... 52 Figure 26 Newly formed bone on lateral implant face and internal thread (arrowed) in Ag AH group ...... 53 Figure 27 Increased frequency of voids (arrowed) and reduced bone-implant contact (boxed) in acid-etched implant group ...... 54 Figure 28 Mean Shear Stress of cortical implants in ovine model at 4 week and 12 week timepoints. Results from current study highlighted in purple (4 weeks) and green (12 weeks). Acid-etch titanium had lower shear stresses than all coated titanium substrates...... 59 Figure 29 Mean Bone Implant Contact of cortical implants in ovine model at 4 week and 12 week timepoints Results from current study highlighted in purple (4 weeks) and green (12 weeks). BIC for PS Ti** was markedly lower than other plasma-sprayed variants...... 60 Figure 32 Mean shear stress of pushout at 12 weeks in ovine model of Ag HA and Conventional HA coatings ...... 86 Figure 33 Mean BIC in cortical bone at 12 weeks for Ag HA and Conventional HA coatings ..... 86
vi List of Tables
Table 1 Study design indicating group (Group 1: Acid-etched, Group 2: Ag HA) and timepoint per implantation site. Femur and Tibia indicate cancellous sites. Cort 1, 2 and 3 indicate cortical sites in descending order from the top of tibia...... 19 Table 2: 4-week Mechanical Testing Results showing calculated p-value for each parameter . 45 Table 3 SPSS Output of Independent t-test for Mechanical Testing at 4 weeks. All parameters were found to be significantly different (p<0.05) between the groups (red boxes), excluding the average cortical thickness of the tested specimens (blue box). This indicates variations can be attributed to the quality bone-implant interface...... 45 Table 4: 12-week Mechanical Testing Results showing calculated p-value for each parameter 46 Table 5 SPSS Output of Independent t-test for Mechanical Testing at 12 weeks. All parameters were found to be significantly different (p<0.05) between the groups (red boxes), excluding the average cortical thickness of the tested specimens (blue box). This indicates variations can be attributed to the quality bone-implant interface...... 46 Table 6 Bone ongrowth evaluation of cortical specimens. Mean percentage ongrowth of the Ag HA implants was consistently higher than that of acid-etched implants at both timepoints. ... 49 Table 7 ANOVA Output for cortical samples, testing bone ongrowth at all timepoints. BIC is dependent upon implant type and timepoint, but variation between groups is independent of time in situ ...... 49 Table 8 Bone ongrowth evaluation of cancellous specimens. Mean percentage ongrowth of the Ag HA implants was consistently higher than that of acid-etched implants at both timepoints...... 50 Table 9 ANOVA Output for cancellous samples, testing bone ongrowth. BIC is dependent upon implant type, but independent of timepoint, and variation between groups is independent of time in situ ...... 50 Table 10 Comparison between current study and previous HA study in same ovine model ..... 84
vii Acknowledgements
I would like to thank Dr. Matthew Pelletier for his constant guidance and expertise throughout the entire duration of this ordeal research project. I am also indebted to Dr. Bill Walsh and Dr. Nicky Bertollo who lent their time, advice and priceless experience to many aspects of this work. I am extremely grateful to Dr. Declan Brazil for going out of his way to make this whole thing possible.
I can’t even begin to express my appreciation for the unwavering support of
Santhara and my family, so I’ll just leave it at that.
Most of all, I want to acknowledge my Seeya, who wanted this for me more than anybody. I know he would have been equal parts thrilled and relieved to see it finally happen.
viii Chapter 1. Introduction
1.1 Infection and revision of orthopaedic implants The popularity of orthopedic implants in surgical interventions is expected to continue its steady increase seen during recent decades, with the demand for primary total hip and knee and knee projected to reach 572,000 and 3.48 million procedures in the USA alone, by 2030 [1]. Similarly, revision surgeries associated with these primary procedures are also set to grow by up to 601%, based on 2005 rates [1]. The economic drains and impact upon patient health associated with a revision procedure has been well documented [2], and as such the developments aimed at improving primary implant success represent a unique and significant challenge in the field.
In Australia, 17.1% of revisions of primary conventional total hip replacements in 2013 were due to infection (n = 1534) [3]. These rates were even higher in primary total knee replacements, with 22.2% of revisions in 2013 due to infection (n = 3038) [3]. Similar trends were observed in the United Kingdom, with 12% of all hip revisions (total 10,040) and 22% of all knee revisions (total
6,009) occurring as a result of infection in 2012 [4].
Although infection represents a major cause of Total Joint Replacement (TJR) revision, the actual incidence of infection as a proportion of all joint replacement procedures remains low. An analysis of NIS data in the USA from
1990 – 2004 conducted by Kurtz et al [5] recorded infection rates of 1.04% for both hip arthroplasties and knee arthroplasties, despite the number of knee arthroplasty revisions being higher (5,838 vs. 3,352 revisions). This calculation did not include arthroplasty devices explanted as the first stage in 2-stage revision procedures to treat infected joints. In 2001, the infection burden 9 (defined as the ratio of revisions for infection to the total number of arthroplasties) was calculated at 1.99% for total hip and 2.05% for total knee arthroplasties. The study data was updated following the release of more recent
NIS data in 2010. By this time the infection burden rates had increased to
2.21% for total hip arthroplasty and 2.32% for total knee arthroplasty, with an average infection burden rate from 2001-2010 of 2.20% for total hip and 2.25% for total knee arthroplasties [6]. The increase may partly be explained by a significant decline in length of hospital stays, which reduces the likelihood of early identification of infection during the initial post-operative stay.
The trends noted in the NIS data reflect similar incidence rates in other global centers. Data from the Australian Joint Registry indicates a cumulative incidence of revision due to infection of approximately 0.6% following primary total hip replacement and 1.0% following primary total knee replacement, up to
13 years after the procedure [3] with further studies recording infection rates within this 0.6% - 2.25% range [7-10]. Infection may occur at any period through the life of the implant, however it is generally observed that the vast majority of infections develop within the one to two years postoperatively [8-
12].
1.2 Economic impact of prosthetic infection Despite the low incidence of infection when compared to the total number of joint replacement procedures performed, treatment and revisions for infected prostheses are a costly, resource intensive exercise, particularly when compared to revisions for other causes such as loosening. The financial burden associated with infection of total joint replacements has been well documented.
10 Klouche et al [13] performed a retrospective analysis of 424 primary THA, 57 non-infected THA revisions and 40 THA revisions due to infection. The study examined the medicosurgical costs of each treatment, considering human resources, prescriptions, medicotechincal and service costs. Revision of the infected THA cost 3.6 times more than the primary procedure, whilst an aseptic revision was 1.4 times the primary procedure. Revisions for septic devices also required longer hospital stays (mean 30.6 days) when compared to an aseptic revision (8.9 days). Similar results were obtained in a study by Peel et al [14], examining both hip and knee procedures, which demonstrated the cost of managing a prosthetic joint infection case was 3.1 times the cost of the primary arthroplasty. Treatment and management of infection entailed greater number of re-admissions, more additional surgery, longer hospital stays (31.6 days vs.
7.9 days), with a mean cost of $69,414 compared with $22,085. Similar increases in financial burdens are documented in economic studies by Kapadia et al in the US and Garrido-Gomez et al in Spain [15, 16]. It is estimated that in the UK alone, the cost of infected revisions to the NHS is in the order of £200 million per annum [17].
1.3 Mechanisms of prosthetic infection Given the devastating impact of prosthetic joint infection on patient outcomes, and the difficulty and cost of treatments or revision, significant developments have been made to create strategies aiming to prevent infections in the surgical setting. This includes advances in operating standards, patient isolation to confine pathogenic strains, control of potential personnel and environmental sources of contamination during surgery, as well as peri-operative prophylaxis to combat infection establishment [18, 19]. Whilst effective, these strategies do 11 not directly address the ongoing issue of bacterial adhesion to implant materials, which serves as the genesis of periprosthetic joint infections.
The mechanisms of periprosthetic joint infection differ from other forms of systemic infection, due to the presence of an inanimate biomaterial substrate.
Whilst biomaterials are not biologically inactive at an atomic level, they are inanimate and therefore present a surface susceptible to colonisation by opportunistic bacteria [20]. The surrounding regions of an implant are known to have local immune depression, which further increases the vulnerability to microbial colonization [21, 22]. In orthopaedic applications, damaged or traumatised tissues caused by wear particles or friction at the implant surface are also, by extension, inanimate substrates susceptible to microbial colonisation, and subsequent development of infection [20, 23]. The presence of a foreign material has also been shown to dramatically reduce the dose of contaminating microorganisms required to cause infection at the site, up to a factor of 100,000 times in one animal study [24-27].
Generally, organisms responsible for infection originate from the skin flora of the patient or physician during the procedure, which enter the open wound and migrate through incision channels to the implant surface [22, 28]. The microorganisms most commonly responsible for infection have been identified as coagulase-negative staphylococci (CoNS) and S. aureaus, which together reportedly account for approximately 50-65% of infection cases [26]. An evaluation by Campoccia et al [23] of nearly 800 clinical isolates from prosthetic infections since 2000 found that roughly four out of five infections were caused by staphylococci, whilst S. aureas and S. epidermidis specifically accounted for
12 34% and 32% of infection isolates respectively.
Implant infection is instigated by initial bacterial adhesion to the biomaterial surface [22]. Surfaces exposed to the biological environment immediately acquire a film of proteins, which attract bacteria as a source of nutrition.[20,
22]. Subsequent prosthesis-specific infection requires active interaction between the biomaterial surface and the bacteria. This can include the bacterial production of surface adhesins which attach to the protein films on the implant, or production of a polysaccharide “slime” to create an adhesive biofilm on the implant surface [22, 23, 28-30]. Biofilm contains a multi-level community of bacteria more protected from the host immune system, and which are less susceptible to conventional antimicrobial agents [22, 23, 28]. Isolation of biofilms on infected hip prostheses has identified CoNS, S. aureaus as well as other microorganisms present [31].
The unique pathogenesis of prosthetic joint infection has driven the development of preventative strategies targeting the tissues surrounding the implant/biomaterial interface. This site represents the area of initial bacterial adhesion to the implant, which is a crucial step in the development of infection
[23]. Current developments focus upon alteration of the outer-layer chemistry or surface topology of the biomaterial, to disrupt initial microbial adhesion whilst maintaining the required mechanical and biocompatible properties of the material. Potential surface modifications include coatings with surfactants or proteins to create adhesion resistant surfaces, as well as bioactive coatings such as chitosan which have large-spectrum antimicrobial properties [32, 33]. The use of a coating doped with silver ions is another example of a bioactive coating,
13 which facilitates controlled elution of metal ions into the interstitial space to help prevent microbial adhesion to the implant surface.
1.4 Antimicrobial properties of silver ions The broad uses of silver ions against microbial action has been utilised for centuries, with current uses in a range of applications including wound dressings, urinary catheters and water systems[34, 35]. Silver is often described as oligodynamic, meaning it is able to generate a bactericidal effect at minute concentrations., with reports of bactericidal activity at concentrations as low as 35 parts per billion [36, 37]. The Ag+ ion is an effective antimicrobial agent as it remains non-toxic to human cells [38] whilst displaying antiseptic properties [39]. When used as a bioactive coating, silver ions have been shown to reduce initial bacterial adhesion and colonisation upon the implant surface, thereby disrupting the development of biofilm [40, 41]. Chaw et al [42] demonstrated that even low concentrations of silver, whilst unable to exhibit antimicrobial effects within biofilms, were capable of destabilizing the biofilm matrix of S. epidermidis bacteria. Similar results have been recorded by Stobie et al [41].
Additionally, controlled elution of ions from the coating can provide an antimicrobial effect in the interstitial joint space surrounding the implant, with the ions performing a bactericidal function. The mode of action of the silver ion is multifaceted, but generally believed to rely upon binding of the Ag+ cation to the negatively charged bacterial cell wall, denaturing the membrane and ultimately leading to loss of structural integrity and function, cell lysis and death [37, 43, 44]. Silver ions are able to bind to molecular groups of enzymes in
14 the cell wall, thereby disrupting key cell metabolic processes such as respiration or ion transport [45]. Once within the bacterial cell, silver ions can further bind to proteins and inhibit cell DNA synthesis and function [46]. The affinity of silver ions to proteins has lead to suggestions that impregnation of silver ions into a coating may be more effective than a direct surface coating alone, as surface silver ions can be readily deactivated by the surface proteins of a device following implantation [41, 47].
Excessive amounts of silver compounds or long term treatment with silver can lead to argyria, a discolouration of skin or tissues, which is otherwise not harmful [48]. Further, silver toxicity or argyrosis can be resolved with the cessation of therapy, which will occur naturally in the case of elution’s from silver coatings on implants [49]. Levels of silver concentration associated with argyrosis are reported to range from 4-6g silver, while in comparison Gosheger et al [50] estimates the silver concentration required for coating a total femoral replacement to be approximately 1.15g, indicating the risk of developing systemic argyrosis is unlikely.
1.5 Use of silver in current implant technology In vivo studies of silver-coated implants have supported the use of silver ions to reduce incidence of periprosthetic infections. An animal study by Gosheger et al
[50] examined the in vivo antimicrobial efficacy of silver coated megaprostheses, and the toxicological side effects of the coating. In this study
30 rabbits were implanted with either a titanium or silver-coated titanium endoprostheses, and subsequently infected with S. aureus. Silver coatings had
99.7% purity, and were applied by galvanic deposition to a layer thickness of
15 10- 15 µm, with a 0.2 µm thick layer of gold to act as a cathode driving the release of Ag+ ions. At 90 days postoperative follow-up, the silver group showed significantly lower infection rates (7% vs. 47% p<0.05) when compared to the titanium group. A second group of 10 rabbits were implanted with silver-coated endoprostheses to evaluate the toxicological side effects of the coating. The results from this group showed elevated silver concentrations in blood and the organs, with no pathological changes in laboratory parameters, or histological change in organs. This indicates that the silver-coating is able to successfully reduce infection rates without adverse toxicological side effects. A similar study by Collinge et al [51] utilised stainless steel pins coated with silver, and implanted in sheep infected with S. aureaus. At 19 days follow-up, 84% of the uncoated pins were infected, compared with 62% of the coated pins.
Additionally, motion of the implants was found to correlate highly with infection at the site, with silver-coated implants displaying much lower quantities of biofilm when examined under electron microscopy.
Early outcomes of the use of silver ions in clinical settings have shown promising results with respect to infection control. A retrospective evaluation conducted at the Royal Orthopaedic Hospital in Birmingham, UK examined the incidence of early periprosthetic infection in high-risk patients treated with silver-treated custom endoprostheses [52]. 170 patients were evaluated in two equal groups, one with silver treated implants and the other a control group, with data collected at 3, 6, 9 and 12-month post-operative follow-up visits. Post- operative infection rates were halved in the silver treated group (11.8% vs.
22.4%). Additionally, treatments for infection were more effective in the silver
16 treated group than controls (success rates with DAIR were 70% vs, 31.6%).
Therefore, mid-term results of the study associated silver-treated endoprostheses with lower rates of early periprosthetic infection, and superior outcomes for subsequent treatments and revisions.
17 Chapter 2. Method
2.1 Study Design Summary Implants were evaluated for osseointegration using a standard bilateral ovine model developed by Walsh and Bruce [53]. This model facilitates both bicortical implantation sites at the tibial midshaft, and cancellous implantation sites at the distal femoral condyle and proximal tibia, within a single animal. A total of
40 implants divided into 2 implant groups were evaluated in this study. Group
1 comprised of the acid etched titanium implants, whilst Group 2 consisted of the silver-doped hydroxyapatite (Ag HA) coated implants. An overview of the study is designed, including implant group used at each site, in presented in
Table 1.
Osseointegration was evaluated at 4-week and 12-week time points. Each time point consisted of 2 animals, for a total of 4 animals in this study. The bilateral ovine model utilises the rear legs of the animal for implantation. Each leg provides 3 bicortical implantation sites and 2 cancellous implantation sites.
Therefore, utilising 2 animals per time point allows 12 bicortical sites (n=12 specimens per group) and 8 cancellous implantation sites (n=8 specimens per group) to be evaluated at each time point.
Implant evaluation at each timepoint comprised of mechanical testing and histomorphometric analysis. Mechanical testing was performed on cortical samples to evaluate the shear stress of pushout from cortical bone. This provides an indication of the strength of the new bone/implant interface and therefore the success of osseointegration of the implant. Histomorphometric analysis allowed the quantification of bone ongrowth along the implant
18 perimeter to compare the extent of osseointegration and bone adhesion in each group per timepoint.
Table 1 Study design indicating group (Group 1: Acid-etched, Group 2: Ag HA) and timepoint per implantation site. Femur and Tibia indicate cancellous sites. Cort 1, 2 and 3 indicate cortical sites in descending order from the top of tibia.
Left Leg Right Leg
Animal Femur Tibia Cort1 Cort2 Cort3 Femur Tibia Cort1 Cort2 Cort3
W2602 1 2 2 1 2 1 1 1 2 1
W2603 1 2 2 1 2 1 1 1 2 1
W2604 1 2 2 1 2 1 1 1 2 1
W2605 1 2 2 1 2 1 1 1 2 1
Shaded cells indicate 4-week timepoint. Remaining cells are 12-week timepoint.
2.2 Implant Manufacture Two titanium implant groups were evaluated for osseointegration in this study.
All implants consisted of a Ti6Al4V substrate, in the form of a cylindrical dowel
20mm in length. Dowels intended for Group 1 (acid etching) had a dimeter of
6mm, whilst dowels intended for Group 2 (Ag HA coating) had a diameter of
5.6mm. The 0.4mm reduction in diameter of the Group 2 implants was intended to allow the application of the Ag HA coating to a target thickness of
0.2mm, such that final implant diameter remained constant across both groups.
A standard M4 metric thread was tapped longitudinally into all dowels to a depth of 5mm, which facilitated the attachment of instruments required for the surgical implantation of the devices. A total of forty (40) Ti6Al4V dowels were manufactured for this study by Signature Orthopaedics Ltd (Sydney, Australia) before undergoing further processing, such as surface treatments, coating applications and sterilisation. 19 Group 1 (acid etched) implants were not coated, but subject to a proprietary nanotexturing process of the Ti6Al4V substrate through exposure to an acid by
KKS Ultraschall AG (Steinen, Switzerland). All external surfaces of the dowel were exposed to the acid etching process. Group 1 contained 20 implants in total.
Group 2 (Ag HA coating) implants first underwent additional processing in the form of grit-blasting of the external cylindrical surface. Subsequently, they were plasma-sprayed with a silver-doped hydroxyapatite (Ag HA) coating by
Accentus Medical (Didcot, UK) which covered all external surfaces of the dowel, excluding the cylindrical end face surrounding the threaded hole. The coating was applied to a target uniform thickness of 0.1mm through proprietary processes developed by Accentus Medical, to ensure the diameter of the final coated implant was 6mm. Group 2 also contained 20 implants in total.
Following final processing all implants were provided non-sterile by the respective suppliers. Initial SEM imaging was performed to evaluate and compare the implant surfaces prior to implantation. Imaging was completed using a Hitachi S-3400 SEM (Hitachi High-Technologies Corporation, Tokyo,
Japan), with images taken up to 1000x magnification at various points along the implant.
Implants underwent a final cleaning process at Signature Orthopaedics Ltd before sterilisation through gamma irradiation from 25-40 kGy (Steritech Pty
Ltd, Narangba, Australia). Implants were therefore provided at surgery clean, sterile and individually packed.
20 2.3 Animal Preparation Four skeletally mature sheep (cross-bred Merino Wethers, 18 months) were used in this study with ethical consent from the institutional Animal Care and
Ethics Committee. Each animal was fasted from both food and water for 24 hours prior to undergoing the surgical procedure. Animals were rendered unconscious via an intramuscular injection of Zoletil (Virbac, Carros, France), whilst they remained in the holding pen, on the day of the surgery. When the animal had lost consciousness, it was position in a left lateral position with neck extended upon on a table for subsequent intubation. An 8.5Fr endotracheal tube was introduced and the cuff was inflated with 10mLs of air, whilst the tube was fastened securely to the lower jaw of the animal. Animals were given 02 at a rate of 4L/min and 1.5-2.5% Isoflurane using an anaesthetic machine. Throughout the procedure, animals continued to receive the above, as well as 1g of Cephalothin (intravenous) and 5mLs of Bencillin as antibiotic prophylaxis (intramuscular, Troy Laboratories, Glendenning, Australia).
Animals further received 4mLs of Carprofen (Rimadyl, Zoetis, NJ, USA) and
1mL of buprenorphine (Temgesic, 0.324mg) to provide pain relief prior to the surgical procedure.
2.4 Cortical Site Implantation Bicortical implantation sites were selected along the tibial mid-shaft of the rear legs of each animal. A 3cm surgical incision was made approximately 50mm from the articular surface along the anteromedial aspect of the tibia. Following exposure of the periosteum, further dissection was performed to visualise the underlying cortical bone of the tibial diaphysis. Bicortical implants were implanted in a line-to-line scenario. Therefore, a bicortical hole was created
21 using increasing drill diameters up to a maximum of 6mm. A threaded insertion instrument and surgical hammer were then used for impaction of the implant into the implantation site. The implant was impacted until it was flush with the surface of the cortical bone, as shown in Figure 1. This procedure was repeated for the remaining two bicortical implants, with a spacing of 20mm between implantation sites. The surgical site was finally closed using resorbable sutures.
Figure 1 Three cortical implants in tibial diaphysis of animal W2603 showing implant flush with bone surface
Due to slight variations in coating thickness of the Group 2 Ag HA implants, it was observed that some Group 2 implants were more difficult to impact into the line-to-line implantation scenario than others. All implants were subject to final inspection by the suppliers prior to receipt. However, the dimensional tolerance of ±0.1mm on the thickness of the Ag HA coating may have contributed to the tactile variation in ease of insertion.
22 2.5 Cancellous Site Implantation Cancellous sites were chosen at the medial aspect of the distal femoral condyles and proximal tibia. A 1cm incision was made and muscle dissected to expose the bone beneath. Cancellous implants were evaluated in several different implantation scenarios encompassed within a single implantation site. These included press-fit (interference), line-to-line, a 1mm gap and 2mm gap either side of the implant. Multiple implantation scenarios were achieved by the use of a step drill, as shown in Figure 2 and Figure 3. This drill incorporated stepped diameters of 4mm, 6mm, 8mm and 10mm along its length, providing the required hole diameters for the implantation scenarios described. Note that the press-fit (interference) scenario was achieved by over drilling the step- drilled hole using a 5.5mm drill bit resulting in steps at 5.5mm, 6mm, 8mm and
10mm.
Figure 2 Implantation overview of ovine model showing four implantation scenarios in cancellous sites and line-to-line implantation in bicortical sites [54]
23 Implants were inserted using a threaded insertion instrument and surgical hammer for impaction into the implantation site, until flush with the surface of the cancellous bone. Following implantation, tissues were reflected and the site closed with resorbable sutures. There were no complications associated with the implantation of the cancellous implants.
Figure 3 Step drill used in surgery to provide a range of implantation scenarios within a single site
2.6 Post-operative Recovery Following completion of the surgery, animals were allowed to rest until they were deemed to be breathing independently of the anaesthetic machines. The endotracheal tube was removed when the animal was consciously chewing on the tube. Animals were initially transferred to a cage until they sufficiently recovered to attain a standing position. At this point, they were deemed fit to be transferred to pen, shared with another sheep, and with feed and water supply.
Animals were observed in their pen environment to ensure they were recovering appropriately from the surgical procedure. Any signs of infection,
24 haematoma or swelling, bleeding or ill health could indicate issues associated with the implantation. Within the pen, animals were allowed to move unrestricted and with full weight bearing, without the use of splints. Post- operative analgesic relief was provided for the first two days following the surgery, in the form of 4mls of Carprofen, SC. One animal, W2604, showed signs of a haematoma approximately 5cm in diameter on the right tibial midshaft. However, this did not appear to impede the animal’s mobility or present distress.
2.7 Harvest and Sample Preparation At the required time point, animals were euthanised through an overdose of sodium pentobarbitone (Lethabarb, Virbac, Australia) delivered by lethal injection to the jugular vein. The cull was confirmed by an absence of muscular twitches of the eyelids in response to finger clicking and other auditory stimuli.
Animals were transferred to the University wet labs where the hindlimbs of the animals were harvested through direct separation at the hip joints. The lungs, liver, kidneys and spleen of each animal were also harvested, with no evidence of adverse reactions noted. All external tissues including skin, muscles and ligaments were systematically stripped from the harvested limbs using a scalpel, in order to isolate the femur and tibia containing the surgical implantation sites, as shown in Figure 4.
25 Figure 4 Isolated femur and tibia (both left and right) from animal W2603
Following the removal of soft tissues to isolate the femoral and tibial bones, radiographs of the harvested bones were taken using a Faxitron (Faxitron,
Wheeling, IL) with digital plates (Agfa Healthcare, Mortsel, Belgium). Two X- rays were taken, in the anteroposterior and lateral views, encompassing the 5 implantation sites on each hindlimb.
Each individual implant was then isolated from the main bone in order to undergo the required mechanical testing and subsequent SEM imaging. The harvested bone was sectioned into several segments, each containing one implant. Sectioning was performed by hand using a band saw to cut axially through the bone at the required points. Cancellous implants from the femoral and tibial condyles were isolated to include the entire implant and surrounding bone. These cancellous samples were placed immediately into a glass jar and fixed in cold phosphate 10% buffered formalin, to facilitate further testing at a later date. 26 Cortical implants were initially isolated in three axial segments taken from the tibial midshaft, as shown in Figure 5. All axial segments included the bicortical ring of tibial bone, and generally elements of internal bone tissues and marrows.
Figure 5 Isolated axial segment from tibial diaphysis containing cortical implant
The axial segments of the cortical implants then underwent further processing in preparation for sectioning into medial and lateral specimens. The superior and inferior surfaces of cortical bone surrounding the implant were subject to grinding and polishing, to ensure they were parallel to implant in the sagittal plane. These parallel surfaces allowed the cortical bone to be mounted in the
Bueler low speed saw, such that the implant was fixed perpendicular to the diamond-coated wafering blade. The Bueler low speed saw was then used to section each cortical implant into medial and lateral halves, as shown in Figure
6.
27 Figure 6 Sample W2602L4 following sectioning, showing medial half (W2604L4-M)
2.8 Mechanical Testing Cortical implants were mechanically tested to evaluate the shear strength of the bone-implant interface at each time point. At the 4-week time point, mechanical testing was performed on both medial and lateral cortical implant specimens i.e. 12 samples per group. At the 12-week time point, mechanical testing was performed only on the medial cortical implant specimens, i.e. 6 samples per group. The lateral cortical implant specimens of the 12-week time point were not used in pushout testing in order to preserve the bone-implant interface for SEM analysis of the interaction between the implant surfaces and surrounding bone.
Prior to pushout testing, samples were further processed to remove periosteal bone surrounding the implant, and create a flat face of cortical bone perpendicular to the axis of the implant. This was achieved through polishing
28 of the specimen, until the outermost circular face of the implant was flush with the surface of the cortical bone. Removal of the periosteal bone was crucial in ensuring there was no residual bone impeding the progress of the implant, such that the measured force during the pushout test relates entirely to the shear interaction between implant and bone, rather than axial obstruction with periosteal bone.
Following sample preparation, the cortical bone thickness of each specimen was measured using digital callipers at two locations either side of the implant, and recorded for pending shear stress calculations.
Specimens were loaded onto the test bed of a calibrated uniaxial servohydraulic test machine (858 Mini Bionix ®, MTS Systems Inc, Minneapolis, Minnesota,
USA). Specimens were placed on a 5mm thick stainless steel support jig containing an 8mm hole, which would capture the implant upon pushout from the cortical bone. Specimens were placed face down upon the flat surface ground perpendicular to the implant, such that the implant was now vertical along its longitudinal axis. Above the specimen, a stainless steel push-out pin was attached to the actuating arm of the MTS unit. The push-out pin included a 6mm spigot designed to contact the implant’s axial circular face, and generate the pushout force. Specimen were aligned such that the implant was directly below the push-out pin and situated over the hole in the support jig, with a minimum distance of 1mm between the edge of the hole and the implant.
The MTS unit was programmed to apply a compressive axial force upon the implant via the push-out pin, at a rate of 0.5mm/min. Axial load and displacement data was captured at a sampling rate of 50Hz. The axial force was 29 applied until a peak pushout load was achieved, indicated by increasing applied displacement with decreasing load. Recorded data was evaluated by plotting the overall force-displacement curve of each specimen, to present the peak shear force during pushout. Further calculations using this data were performed to evaluate stiffness, energy to failure and proof resilience using a custom script developed for Matlab R2009a (Mathworks Inc, MA, USA).
2.9 SEM Sample Preparation All samples, both cancellous and cortical, were embedded in polymethylmethacrylate (PMMA) in preparation for SEM imaging and histology analysis. Prior to fixation in PMMA, samples were initially placed in jars of 10% cold phosphate buffered formalin. For cancellous specimens, this was done immediately after isolation of each implant from the harvested bone.
For cortical specimens, this was done following pushout testing. The 12-week lateral cortical implants which did not undergo mechanical testing were placed in the formalin immediately after sagittal sectioning into the medial and lateral halves.
After the initial 10% buffered solution, samples were transferred through a series of containers containing increasingly concentrated ethanol solutions, in order to sequentially dehydrate the specimens. Specimens were held in each concentration of ethanol for 7 days, before transfer to incrementally higher concentration from 70% to 100%. Following dehydration, specimens were polymerised in PMMA and allowed to cure for several days before further processing.
30 Embedded samples underwent further preparation to facilitate imaging via
SEM. From their embedded state, the implant surfaces were isolated to exposed along the longitudinal axis such that the bone-implant interface could be assessed. The embedded samples were initially processed using the band saw to rapidly remove material not required for evaluation including PMMA and excess bone and tissue. Care was taken not to damage the implant with the band saw blade, and to maintain sufficient PMMA for clamping in fixtures and jigs during later processing stages.
Specimens were subsequently loaded onto the Bueler low speed saw, and aligned with the wafering blade such that the implant would be sectioned along its longitudinal axis. The initial sectioning was then performed to divide the implant into two halves. Following the initial sectioning, the sample was translated 450µm to allow a second, parallel cut to be made. The end result was a section of embedded implant, with a thickness of 450µm, exposing the bone- implant interface along the longitudinal midline of the implant.
A thickness of 450 µm was chosen as it has previously been demonstrated to be an effective thickness for imaging embedded samples through SEM, without excessive distortion caused by the PMMA medium. Following sectioning, the implant face of all SEM specimens was polished using a fine grade of polishing paper to enhance the clarity of the SEM image and reduce the likelihood of artefacts or “cloudiness” during subsequent SEM imaging.
31 2.10 SEM Imaging Specimens were assessed with back scattered electron microscopy (BSEM) imaging on a Hitachi S-3400 SEM (Hitachi High-Technologies Corporation,
Tokyo, Japan). Each implant required a series of images to cover both the upper and lower perimeter of bone-implant contact regions. The number of images required varied from four to six, depending on the magnification selected to provide the clearest image for histomorphometric analysis.
Magnification was varied between 40x and 80x across all samples in both timepoints. Examples of the image series used are presented in Figure 7.
Images were saved for subsequent histomorphometric analysis.
Figure 7 Raw SEM image of Specimen W2604R5L at 80x magnification. Implant (blue arrow) is displayed as white, while bone (red arrow) is displayed as grey. Voids (circled) are represented as darker regions.
32 2.11 Histomorphometry SEM images were evaluated to quantitatively define the extent of bone
ongrowth for each specimen, as a percentage of the total bone-implant
interfacing perimeter. The SEM images highlighted metal as white, voids as
black, and bone/coating materials as shades of grey. An existing in-house script
for MATLAB R2009a (Mathworks Inc, MA, USA) was used to identify the bone-
implant interface of each image and calculate the total length of the perimeter,
using the variation in pixel colour corresponding to various structures within
the image. Regions of bone ongrowth or bone voids were manually defined by
the operator along the length of predetermined perimeter. The script then
calculated the percentage of perimeter designated to have bone ongrowth
present, as a function of the total length. Figure 8 presents an example of an
SEM image following histomorphometric analysis, with the final ratio of bone
ongrowth to total bone-implant interface presented in the top-left corner (0.825
in the example pictured).
Figure 8 SEM images of Specimen W2604R5L showing raw (top) and processed (below) versions. Green represents regions of bone contact, red represents bone voids. Total bone contact is 85.2%, as indicated in top left corner of processed image. 33 2.12 Histology Embedded samples selected for histology analysis were sectioned using a SP
1600 Microtome (Leica, Germany). After mounting the specimen, an initial planed section was performed to ensure the superior surface of the sample was perfectly flat. A glass slide was secured to the sample using a UV adhesive
(Loctite, Dusseldorf, Germany) and a subsequent sectioning was performed to create a 30µm thick section. The section was then cleaned and stained using methylene blue and basic fuschin to highlight bone and fibrous tissues. Two histology sections were taken from each selected sample.
Histology slides were viewed under a light microscope (Olympus, Tokyo, Japan) to observe new bone formation and cell characteristics at both the immediate implant-bone interface, as well as the surrounding extremities of the specimens.
34 Chapter 3. Results
3.1 SEM Coating Characterisation Scanning electron microscopy of the two implant surface topologies are presented in Figure 9 to Figure 12, for two magnification levels, prior to implantation.
Figure 9 SEM imaging of acid etched surface (Group 1) (x50 magnification). Texturing and evenly distributed ridges achieved through acid-etching process visible
Figure 10 SEM imaging of Ag HA (Group 2) coating (x50 magnification). Unique surface of plasma-spray coating visible in the form of compact undulations and microstructures. 35 Figure 11 SEM imaging of acid etched surface (Group 1) (x1000 magnification). Network of ridges, crevices and nanopits visible at this level of magnification.
Figure 12 SEM imaging of Ag HA coating (x250 magnification). Small voids and porous regions visible between the plasma-sprayed structures of the Ag HA coating. 36 At both magnification levels, there is a clear distinction in surface topologies of each group, as it to be expected when comparing a coated and uncoated surface.
Under 1000x magnification the nanotextured features of the acid-etched implant, including large ridges and a smaller network of nanopits and crevices can be clearly observed. Contrastingly, the plasma-sprayed surface of the Ag
HA coating upon the titanium substrate has resulted in a thicker surface coating with an undulating structure creating larger voids and prominences in a random distribution. The addition of elemental silver to the hydroxyapatite coating was not observed to result in an observable variation in surface structure or topology when compared to a conventional plasma-sprayed HA coating.
3.2 Surgery and Harvest There were no complications or issues arising from the surgical procedures or subsequent harvest at the designated time points, as described in the Method.
As previously noted, a haematoma was observed on the right hind limb of animal W2604 prior to harvest at the 12-week end point. However, this did not appear to impede mobility or cause any distress to the animal, therefore no further action was deemed necessary.
Following euthanisation of the animals, the right and left hind limbs were harvested and photographed for later reference. Upon removal of the surrounding skin and tissues from the bones, the implantation sites were clearly visible beneath the surface of tissue at both cortical and cancellous sites, as shown in Figure 13. There were no signs of infection or adverse reactions e.g.
37 discolouration or coating debris associated with the introduction of the implants into the animal’s limbs.
Figure 13 Harvested tibia from W2605 showing visible cancellous (blue arrow) and cortical (red arrow) implantation sites. Not evidence of foreign body reaction or implant rejection surrounding implants in situ
3.3 Radiography
Radiographs of the isolated femoral and tibial bones were taken in the anteroposterior and lateral views, encompassing all 5 implant sites on each limb. The X-Ray images were useful in confirming implant positions and alignment, as well as verifying the absence of post-operative fracture. There were no significant differences noted in the radiographs alone between implant groups at either time point.
Figure 14 to Figure 21 presents the radiographs of the harvested limbs in this study. All radiographs present the isolated femoral and tibia components from each animal. No irregularities or complications were noted upon review of the radiographs.
38 Figure 14 Left limb radiographs of animal W2602, AP(left) and lateral (right) views, showing good implant alignment at all sites
Figure 15 Right limb radiographs of animal W2602, AP(left) and lateral (right) views, showing good implant alignment at all sites
39 Figure 16 Left limb radiographs of animal W2603, AP(left) and lateral (right) views, showing good implant alignment at all sites
Figure 17 Right limb radiographs of animal W2603, AP(left) and lateral (right) views, showing good implant alignment at all sites
40 Figure 18 Left limb radiographs of animal W2604, AP(left) and lateral (right) views, showing good implant alignment at all sites
Figure 19 Right limb radiographs of animal W2604, AP(left) and lateral (right) views, showing good implant alignment at all sites
41 Figure 20 Left limb radiographs of animal W2605, AP(left) and lateral (right) views, showing good implant alignment at all sites
Figure 21 Right limb radiographs of animal W2605, AP(left) and lateral (right) views. Implant alignment was sufficient at all sites.
42 3.4 Mechanical Testing Sectioned cortical implant specimens were subject to pushout testing to evaluate the shear strength of the bone-implant interface. At the 4-week time point, both medial and lateral cortical specimens underwent mechanical testing. At the 12-week time point only medial cortical specimens were mechanically tested, in order to preserve the bone-implant interface of the lateral specimens for further evaluation through SEM and histomorphometry.
Shear stress (N/mm2, i.e. Pa) was defined as the peak axial pushout force acting over the total bone-implant contact surface area. Contact surface area was calculated as the cylindrical surface area of bone surrounding each implant, given by: