The study was supported by the NIH P30AR069655 and R01AR070613 (H. A. A.).

Animal studies were approved by The University of Rochester Committee of Animal Resources. The mice used in this study were C57BL/6 males and females ranging from age 24-29 weeks of age. Mice were housed in standard conditions with food and water ad libitum. Upon euthanasia via carbon dioxide inhalation, followed by cervical dislocation, 20 right femurs (10 male and 10 female) were harvested and frozen at -20 &#176;C until tested.
1. Creation of custom 3D printed mounting guides
NOTE: This step might be needed because different strains and genetic phenotypes might have different anatomical geometries.
<ol>
	<li>Obtain &#181;CT scans of the representative samples.
	<ol>
		<li>Scan representative samples on a &#181;CT scanner with the following settings: 55 kV, 145 &#181;A for 300 ms integration times, and resolution of 10.5 &#181;m voxels.</li>
		<li>Ensure that the captured region covers the proximal end of the femur and continues down through the midshaft. 
		NOTE: If a &#181;CT scanner is unavailable, 2D planar X-rays of the representative samples can be used.</li>
	</ol>
	</li>
	<li>Analyze the &#181;CT scans.
	<ol>
		<li>Using the representative set of &#181;CT scans, obtain a 2D rendering of the anterior view of the proximal femur.
		<ol>
			<li>Obtain &#181;CT images with a resolution of 10.5 &#181;m voxels from the midshaft to the proximal end of the femur. Compile these slices using software (see Table of Materials) into a 3D rendering of the sample.</li>
			<li>Determine a threshold to distinguish bone from the surrounding tissue and apply a Gaussian filter for noise reduction.</li>
			<li>Orient the 3D renderings to eliminate off-axis tilt and ensure that the femur&#39;s anterior surface is viewed.</li>
			<li>Export this 2D view of the 3D rendering as an image file, such as .jpg or .png.</li>
		</ol>
		</li>
		<li>Using an image analysis software (see Table of Materials), measure the femoral shaft angle by drawing a line perpendicular to the femoral shaft 7 mm distally and a second line through the peak of the greater trochanter to the midpoint of the aforementioned perpendicular line (Figure 1).</li>
		<li>Along the 7 mm distal perpendicular line, measure the femoral shaft diameter below the third trochanter.</li>
	</ol>
	</li>
</ol>
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/63394/63394fig01.jpg" /> 
Figure 1: &#181;CT analysis. &#181;CT images of femurs of C57Bl/6 mice are used to calculate the average shaft angle, measured from the top of the greater trochanter through the center of the midshaft, ~7 mm distally. The midshaft diameter was also measured at this position. The 3D renderings of the proximal femur were oriented in an anterior view to display the profile of the third trochanter. The average shaft angle was 93.13&#176; (SD = 1.19&#176;), and the average midshaft diameter was 1.53 mm (SD = 0.14 mm) (n = 20). Scale bar = 1 mm. <a href="https://www.jove.com/files/ftp_upload/63394/63394fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<ol start="3">
	<li>Create the mounting guides using a 3D modeling software program (see Table of Materials) (Figure 2, Supplementary File 1). 
	NOTE: The guides are rectangular cuboids measuring 6.25 mm x 3.25 mm x 7mm with an angled slot, slightly larger than the average shaft diameter determined in step 1.1.2. The angle of the slot will create a consistent angle of 20&#176; from vertical. The guides should be consistent in length, height and width, but can be made with various slot diameters to accommodate anatomical differences among the bone samples.</li>
</ol>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/63394/63394fig02.jpg" /> 
Figure 2: Designing the guides. (A) 3D sketch and (B) visualization of midshaft angling fixture before 3D printing. Based on previous literature, a midshaft angle between 20&#176; maximizes the stiffness. It minimizes the maximal bending moment in the femoral shaft to ensure fractures occur in the neck and variability in mechanical outcomes5. To compensate for the 3.13&#176; deviation from perpendicular in the midshaft average angles, the fixture angle was set to 73.13&#176; to produce an angle of 20&#176;. Alignment fixtures were printed with diameters ranging from 1.9-2.2 mm to ensure a proper fit for varying midshaft diameters. <a href="https://www.jove.com/files/ftp_upload/63394/63394fig02large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<ol start="4">
	<li>Using a 3D printer, print the guides. The guides can remain on during the testing process, so printing multiple replicates of the guides can be beneficial for preparing multiple samples at once.</li>
</ol>
2. Sample preparation
<ol>
	<li>Harvest the mouse femurs by making a transverse incision entirely around the mouse abdomen and removing the tissue from the incision to the ankles. Following this, locate the hip socket and carefully use the tip of a pair of fine forceps to dislocate the hip. Cut the additional soft tissue to remove the leg from the mouse.</li>
	<li>Once the leg is harvested, use a scalpel to dislocate and cut through the knee joint. Manually clean the femurs of all soft tissue using forceps, scalpels, and paper towels.</li>
	<li>Test the harvested samples immediately or store them at -20 &#176;C for up to 6 months. If samples are frozen, allow them to come to room temperature and hydrate in PBS for 2 h before prepping.</li>
	<li>Using &#188;&#34; x &#188;&#34; square aluminum tubing (see Table of Materials), cut tubing sections &#189;&#34; to 1&#34; in length. Using an etching tool, label each aluminum segment with the sample IDs.</li>
	<li>Fill half of the tubing segments with putty. Place these tubing segments into a fixture to hold them upright.</li>
	<li>Place the cleaned femurs into the 3D printed guides. To do this, place the samples flat on the benchtop so the anterior surface is facing up. Place the guide directly below the third trochanter, where the shaft diameter becomes more consistent. 
	NOTE: This will leave ~7mm of the proximal femur above the guide.</li>
	<li>To prevent the femur from rotating to the lateral or medial side while placing on the guide, hold the proximal and distal ends with one hand when applying the guides, firmly press the femur onto the workbench and using your other hand, place the 3D printed guide on the midshaft of the femur. Ensure to apply the appropriate diameter guide gently, as the midshaft of the femur can snap if forced into a guide too small.</li>
	<li>Once the guides are on the femurs, place them in front of the corresponding aluminum segments. Using bone cement or other hardening agents, fill the aluminum segments until just full, leaving a little room for displacement.</li>
	<li>Place the femurs with guides on in the correct aluminum segment. 
	NOTE: The guides will not be centered on the aluminum segments, seated slightly to one side to allow the distal end of the femur to sit in the center of the aluminum pot.</li>
	<li>Allow the hardening agent to set. Once set, place the samples in a Petri dish with room temperature phosphate-buffered saline (PBS) and allow to rehydrate for 2 h (Figure 3).</li>
</ol>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/63394/63394fig03.jpg" /> 
Figure 3: Sample preparation using custom jigs and angling fixtures. (A) Samples in aluminum pots with the proper alignment are maintained using the 3D printed guides while the bone cement is drying. (B) X-ray before testing shows the shadow of angling fixtures and complete coverage of bone cement surrounding the distal end of femurs. The saturated white area at the bottom of the aluminum pots is putty, used to keep bone cement in pots when hardening. Scale bar (Panel B) = 5 mm. <a href="https://www.jove.com/files/ftp_upload/63394/63394fig03large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
3. Hardware set-up
<ol>
	<li>Using a mechanical testing system (MTS), attach and calibrate a load cell with resolution &#60;1 N (see Table of Materials) (Figure 4A). 
	NOTE: The load cell can be mounted on the stage or, preferably, the actuator when possible.</li>
	<li>Attach a fixture with a square slot that will firmly hold the aluminum segments with the samples. Attach set screws to the two sides of the holding fixture to firmly hold samples in place. (Figure 4B). 
	NOTE: This fixture can be 3D printed or machined and then tapped with threaded screw holes to mount to the testing frame.</li>
	<li>Attach a loading platen to the actuator. This can be simply a tapered screw with a flattened tip (Figure 4C).</li>
	<li>Place a stereomicroscope on a table or surface directly in front of the MTS. If additional lighting is needed to see the set-up through the microscope, place these around the system.</li>
</ol>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/63394/63394fig04.jpg" /> 
Figure 4: Hardware set-up. (A) Set-up of testing on mechanical testing system, with 1 kN load cell (resolution &#60; 1 N) and black biaxial stage to ensure proper sample positioning. (B) Close up of the 3D printed mounting fixture attached to the load cell with an M10 threaded rod and two M4 bolts used to hold the aluminum pot in place. (C) View of the sample through a stereo microscope with a tapered loading fixture. Scale bar (Panel C) = 5 mm. <a href="https://www.jove.com/files/ftp_upload/63394/63394fig04large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
4. Software set-up
<ol>
	<li>In the MTS software, begin the creation of a new flexural (bending) protocol. Ensure that the protocol will operate in displacement control.</li>
	<li>Set the loading rate of the protocol to 0.5 mm/s.</li>
	<li>If the software has a setting for soft keys, add the soft keys &#34;Balance&#34; and &#34;Zero Extension&#34; to the protocol. 
	NOTE: This will quickly set the load and actuator position to 0 before testing each sample.</li>
	<li>Ensure that the software program will record the time in seconds, load in Newtons, and extension or displacement in millimeters at a minimum sampling rate of 100 Hz.</li>
	<li>Save the new protocol and return to the main screen of the software program to begin testing a new sample set.</li>
</ol>
5. Testing set-up
<ol>
	<li>Before mounting the specimens on the MTS, obtain an X-ray image of the samples in the aluminum pots. Multiple samples can be imaged at once. Ensure that the anterior view of samples is captured to allow for verification measurements of potting angle (Figure 5).</li>
</ol>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/63394/63394fig05.jpg" /> 
Figure 5. Assessment of sample alignment. (A) The shaft angle from vertical is measured from planar digital x-rays. (B) Representative potted femoral shaft angles ranged from 18.11&#176; to 23.99&#176;, with a coefficient of variation (COV) of 7.1% (n = 20). Sex differences due to anatomical variations were not statistically significant, as determined using a one-tailed unpaired t-test (p &#60; 0.05). Scale bar (Panel A) = 1 mm. <a href="https://www.jove.com/files/ftp_upload/63394/63394fig05large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<ol start="2">
	<li>Place the aluminum segment with sample into the holding fixture and tighten set screws.</li>
	<li>Lower actuator/loading platen until it is within a few millimeters of the femoral head. 
	NOTE: Do not preload the sample with any force and be careful not to lower the actuator too quickly, as it is very easy to damage samples.</li>
	<li>Using the stereomicroscope, adjust the biaxial stage to align the position of the femoral head directly underneath the loading platen. Lock biaxial stage in place.</li>
	<li>In the MTS software, zero the position of the actuator and balance the load cell using the soft keys added in step 4.3.</li>
	<li>Begin the loading protocol. Depending on how much space was left between the loading platen and sample, testing will only take 10-30 s.</li>
	<li>After testing, capture another anterior X-ray of the sample. This will be used to discern and document the mode of fracture (Figure 6).</li>
</ol>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/63394/63394fig06.jpg" /> 
Figure 6: X-ray image of samples after testing. All samples fractured in a bifurcated line through the femoral neck and along the femoral neck-shaft attachment (highlighted by the orange circle). Scale bar = 1 mm. <a href="https://www.jove.com/files/ftp_upload/63394/63394fig06large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
6. Data analysis
<ol>
	<li>After data collection, export force and displacement data into software (see Table of Materials) that allows for graphing and mathematical calculations.</li>
	<li>Plot the load vs. displacement for each sample (Figure 7A). Fit a linear approximation to the linear segment of the load-displacement curve. The slope of this linear fit will define the stiffness, a measure of the elasticity of the sample.</li>
	<li>Calculate the additional outcomes such as maximum load, maximum displacement, yield load, displacement at yield point, energy to maximum load, and energy to yield point. 
	NOTE: The yield point can be determined by off-setting the linear approximation determined in step 6.2 by 0.2%6. The point at which the off-set line and the load vs. displacement curve intersect will determine the yield point. In the case of very brittle samples that show little yield, the yield point may be the same as the maximum point.</li>
</ol>

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The authors have nothing to disclose.

This protocol outlines a reliable cantilever bending test for murine femoral necks. The natural cantilever flexure scenario that occurs at the femoral neck is typically not represented in standard 3- and 4-point bending tests5. This testing method is better and more reliably replicates the type of femoral neck fractures experienced by bone fragility patients. The main focus when performing this protocol is eliminating the variability due to inconsistent potting of the femoral shaft. Critically, cl...

Fracture risk is a serious medical concern associated with osteoporosis. Over 1.5 million fragility fractures are reported each year in the United States alone, with fractures occurring in the hip, specifically the femoral neck, as the leading fracture type1. It is estimated that 18% of women and 6% of men will experience a femoral neck fracture in their lifetime2, and the mortality rate at 1 year following the fracture is greater than 20%1. Therefore, mouse models that allow biomechanical testing of the femoral neck can be suitable for studying fragility fractures. Mouse models also offer powerful tools to elucidate translatable cellular and molecular events involved in osteoporosis potentially. This is due to the availability of genetic reporters, gain and loss of function models, and the expansive library of molecular techniques and reagents. Mechanical testing of mouse bones can provide necessary outcome measures to determine bone health, genotypic and phenotypic variations that could explain the etiology of the disease, and assess therapies based on outcome measures of the quality of the bone and the risk of fracture3.
The anatomy of the femoral neck creates unique mechanical loading scenarios, which typically lead to flexural (bending) fractures. The femoral head is loaded in the acetabular socket at the proximal end of the femur. This creates a cantilever bending scenario on the femoral neck, which is rigidly attached to the femoral shaft distally4. This differs from traditional 3- or 4-point bending tests on the femoral mid-diaphysis. While these tests are helpful, they do not replicate the loading that typically leads to fragility fractures in osteopenic and osteoporotic individuals in terms of fracture location or the loading scenario.
To better assess fragility fracture risk in mice, it was sought to improve the reproducibility of cantilever bending tests of murine femoral necks. As theoretically predicted, the loading angle on the femoral head relative to the femoral shaft has been shown to significantly affect the outcome measures5, thereby creating a challenge for reliability and reproducibility of reported outcomes. To ensure proper and consistent alignment of the femurs during sample preparation, guides were designed, and 3D printed based on anatomic measurements made on &#181;CT scans of C57BL/6 mouse femurs. The guides were designed to aid in consistently potting the samples such that the femoral shaft is maintained at ~20&#176; from the vertical loading direction. This angle was chosen because it maximizes the stiffness while minimizing the maximal bending moment along the femoral shaft, which increases the likelihood of femoral neck fractures and leads to more consistent and reproducible testing5. Guides were 3D printed in various sizes to accommodate anatomical differences between samples and used to hold samples in a stable position while potting in acrylic bone cement. The stiffness, maximum force, yield force, and maximum energy were calculated from the force-displacement graphs. This testing method showed consistent results for the aforementioned biomechanical outcome. With practice and the aid of the 3D printed guide, measurement errors due to misalignment can be minimized, resulting in reliable outcome measures.

<table><tbody><tr><td>&amp;frac14;&amp;rdquo; x &amp;frac14;&amp;rdquo; square aluminum tubing</td><td>Grainger</td><td>48KU67</td><td>Cut to lengths of 1/2&quot; to 1&quot; lengths</td></tr><tr><td>1 kN load cell</td><td>Instron</td><td>2527-130</td><td>Any load cell with sub 1 N resolution can be used.</td></tr><tr><td>3.5x-45x Zoom Stereo Boom Microscope</td><td>Omano</td><td>OM2300S-GX4</td><td>Microscope used to precisely line up samples with loading platen.</td></tr><tr><td>3D printed guides</td><td>Custom made</td><td></td><td>Angled slots at 73.13&amp;deg;, with diameters between 1.9 mm and 2.2 mm</td></tr><tr><td>3D printed mount</td><td>Custom made</td><td></td><td>Tapped with M10 threads to fit the mount attachment and with 2 M4 threaded holes adjacent sides to hold the aluminum tubing with sample in place.</td></tr><tr><td>Acrylic Base Plate Material Kit</td><td>Keystone Industries</td><td>921392</td><td>Mix 3.5 g of powder with 2 mL of liquid. This will be enough for approximately 8 samples, and will begin to harden quickly.</td></tr><tr><td>Amira</td><td>ThermoFisher Scientific</td><td></td><td>Used to compile &amp;micro;CT scans</td></tr><tr><td>Biaxial stage</td><td>Custom made</td><td></td><td>Used to center femoral head of sample under the loading platen.</td></tr><tr><td>BioMed Amber Resin</td><td>formlabs</td><td>RS-F2-BMAM-01</td><td>Any resin from formlabs could be used for this project.</td></tr><tr><td>Bluehill 3</td><td>Instron</td><td>V3.66</td><td>Software used to set up loading protocol and collect load, displacement and time data.</td></tr><tr><td>ElectroPuls 10000</td><td>Instron</td><td>E10000</td><td>Mechanical testing system</td></tr><tr><td>Faxitron UltraFocus</td><td>Faxitron BioOptics</td><td>2327A40311</td><td>X-ray imaging system</td></tr><tr><td>Form 2</td><td>formlabs</td><td>F2</td><td>Used to print the mount and guides</td></tr><tr><td>Form 2 Resin Tank LT</td><td>formlabs</td><td>RT-F2-02</td><td>LT Tank was used to be compatible with the BioMed Resin</td></tr><tr><td>ImageJ</td><td>National Institutes of Health</td><td>ImageJ</td><td>Used to assess &amp;micro;CT and X-ray images</td></tr><tr><td>Laxco iLED Series LED Light Source</td><td>ThermoFisher Scientific</td><td>AMPSILED30W</td><td>Light source used in conjugtion with microscope.</td></tr><tr><td>Loading platen</td><td>Custom made</td><td></td><td>This can be any metal rod that is tapered to a diameter of approximately 2.5 mm. We used an M6 screw that was tapered on a lathe.</td></tr><tr><td>Mount attachment</td><td>Custom made</td><td></td><td>To secure the 3D printed mount to the load cell. We used a M10/M6 threaded rod</td></tr><tr><td>Phosphate Buffer Saline (PBS)</td><td>ThermoFisher Scientific</td><td>10010031</td><td>Need to rehydrate the samples once acrylic base plate material has set.</td></tr><tr><td>Plumber&#039;s putty</td><td>Oatey</td><td>31174</td><td>Used to seal the end of the aluminum tubing when pouring acrylic base plate material in. Any clay or putty could be used.</td></tr><tr><td>PreForm</td><td>formlabs</td><td>Preform 3.15.2</td><td>Formlabs software</td></tr><tr><td>Tissue Culture Dish</td><td>Corning</td><td>353003</td><td>Samples can be laid flat in culture dish and covered in PBS to rehydrate.</td></tr><tr><td>vivaCT 40</td><td>Scanco</td><td>&amp;micro;CT 40</td><td>Representative set or actual samples can be scanned prior to printing of guides to calculate femoral shaft angle and diameter.</td></tr></tbody></table>

cantilever bending of murine femoral necks

Fractures in the femoral neck are a common occurrence in individuals with osteoporosis. Many mouse models have been developed to assess disease states and therapies, with biomechanical testing as a primary outcome measure. However, traditional biomechanical testing focuses on torsion or bending tests applied to the midshaft of the long bones. This is not typically the site of high-risk fractures in osteoporotic individuals. Therefore, a biomechanical testing protocol was developed that tests the femoral necks of murine femurs in cantilever bending loading to replicate better the types of fractures experienced by osteoporosis patients. Since the biomechanical outcomes are highly dependent on the flexural loading direction relative to the femoral neck, 3D printed guides were created to maintain a femoral shaft at an angle of 20&#176; relative to the loading direction. The new protocol streamlined the testing by reducing variability in alignment (21.6&#176; &plusmn; 1.5&#176;, COV = 7.1%, n = 20) and improved reproducibility in the measured biomechanical outcomes (average COV = 26.7%). The new approach using the 3D printed guides for reliable specimen alignment improves rigor and reproducibility by reducing the measurement errors due to specimen misalignment, which should minimize sample sizes in mouse studies of osteoporosis.

When potted with the aid of the guide, the femoral shafts were aligned at 21.6&#176; &#177; 1.5&#176;. While this represents &#60;10% deviation from the intended angle of 20&#176;, the coefficients of variation (COV) of the potting angle across all samples tested were 7.6% and 6.5% for male and female mice, respectively (n = 10 per group) as verified by pre-test planar x-rays (Figure 5). Additionally, the post-testing X-rays should be used to assess the mode in which the samples failed. Fail...

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Cantilever Bending of Murine Femoral Necks

The present protocol describes the development of a reproducible testing platform for murine femoral necks in a cantilever bending set-up. Custom 3D printed guides were used to consistently and rigidly fix the femurs in optimal alignment.

Fractures in the femoral neck are a common occurrence in individuals with osteoporosis. Many mouse models have been developed to assess disease states and ...

cantilever-bending-of-murine-femoral-necks

Research

JoVE Journal

Bioengineering

2.1K Views.  University of Rochester Medical Center. De cantilever bending setup die in dit protocol wordt beschreven, creëert een reproduceerbare benadering voor het genereren van femurhalsfracturen, die klinisch relevanter zijn en kunnen worden gebruikt in muizenstudies om naar osteoporose te kijken. Dit protocol creëert een testplatform dat de reproduceerbaarheid verbetert, wat leidt tot een verminderde variatiecoëfficiënt in uitkomstmaten. Daarom minimaliseert het de steekproefomvang die nodig is voor robuuste studies.Begin met h...

Video: Cantilever Bending of Murine Femoral Necks

A Simple Critical-sized Femoral Defect Model in Mice

While bone has a remarkable capacity for regeneration, serious bone trauma often results in damage that does not properly heal. In fact, one tenth of all limb bone fractures fail to heal completely due to the extent of the trauma, disease, or age of the patient. Our ability to improve bone regenerative strategies is critically dependent on the ability to mimic serious bone trauma in test animals, but the generation and stabilization of large bone lesions is technically challenging. In most cases, serious long bone trauma is mimicked experimentally by establishing a defect that will not naturally heal. This is achieved by complete removal of a bone segment that is larger than 1.5 times the diameter of the bone cross-section. The bone is then stabilized with a metal implant to maintain proper orientation of the fracture edges and allow for mobility. 
Due to their small size and the fragility of their long bones, establishment of such lesions in mice are beyond the capabilities of most research groups. As such, long bone defect models are confined to rats and larger animals. Nevertheless, mice afford significant research advantages in that they can be genetically modified and bred as immune-compromised strains that do not reject human cells and tissue.
Herein, we demonstrate a technique that facilitates the generation of a segmental defect in mouse femora using standard laboratory and veterinary equipment. With practice, fabrication of the fixation device and surgical implantation is feasible for the majority of trained veterinarians and animal research personnel. Using example data, we also provide methodologies for the quantitative analysis of bone healing for the model.

Animal models are frequently employed to mimic serious bone injury in biomedical research. Due to their small size, establishment of stabilized bone lesions in mice are beyond the capabilities of most research groups. Herein, we describe a simple method for establishing and analyzing experimental femoral defects in mice.

While bone has a remarkable capacity for regeneration, serious bone trauma often results in damage that does not properly heal. In fact, one tenth of all ...

Medicine

An Intramedullary Locking Nail for Standardized Fixation of Femur Osteotomies to Analyze Normal and Defective Bone Healing in Mice

Bone healing models are essential to the development of new therapeutic strategies for clinical fracture treatment. Furthermore, mouse models are becoming more commonly used in trauma research. They offer a large number of mutant strains and antibodies for the analysis of the molecular mechanisms behind the highly differentiated process of bone healing. To control the biomechanical environment, standardized and well-characterized osteosynthesis techniques are mandatory in mice. Here, we report on the design and use of an intramedullary nail to stabilize open femur osteotomies in mice. The nail, made of medical-grade stainless steel, provides high axial and rotational stiffness. The implant further allows the creation of defined, constant osteotomy gap sizes from 0.00 mm to 2.00 mm. Intramedullary locking nail stabilization of femur osteotomies with gap sizes of 0.00 mm and 0.25 mm result in adequate bone healing through endochondral and intramembranous ossification. Stabilization of femur osteotomies with a gap size of 2.00 mm results in atrophic non-union. Thus, the intramedullary locking nail can be used in healing and non-healing models. A further advantage of the use of the nail compared to other open bone healing models is the possibility to adequately fix bone substitutes and scaffolds in order to study the process of osseous integration. A disadvantage of the use of the intramedullary nail is the more invasive surgical procedure, inherent to all open procedures compared to closed models. A further disadvantage may be the induction of some damage to the intramedullary cavity, inherent to all intramedullary stabilization techniques compared to extramedullary stabilization procedures.

This protocol describes an osteosynthesis technique using an intramedullary locking nail for standardized fixation of femur osteotomies, which can be used to analyze normal and defective bone healing in mice.

Bone healing models are essential to the development of new therapeutic strategies for clinical fracture treatment. Furthermore, mouse models are becoming ...

Biomechanical Testing of Murine Tendons

Tendon disorders are common, affect people of all ages, and are often debilitating. Standard treatments, such as anti-inflammatory drugs, rehabilitation, and surgical repair, often fail. In order to define tendon function and demonstrate efficacy of new treatments, the mechanical properties of tendons from animal models must be accurately determined. Murine animal models are now widely used to study tendon disorders and evaluate novel treatments for tendinopathies; however, determining the mechanical properties of mouse tendons has been challenging. In this study, a new system was developed for tendon mechanical testing that includes 3D-printed fixtures that exactly match the anatomies of the humerus and calcaneus to mechanically test supraspinatus tendons and Achilles tendons, respectively. These fixtures were developed using 3D reconstructions of native bone anatomy, solid modeling, and additive manufacturing. The new approach eliminated artifactual gripping failures (e.g., failure at the growth plate failure rather than in the tendon), decreased overall testing time, and increased reproducibility. Furthermore, this new method is readily adaptable for testing other murine tendons and tendons from other animals.

The protocol describes efficient and reproducible tensile biomechanical testing methods for murine tendons through the use of custom-fit 3D printed fixtures.

Tendon disorders are common, affect people of all ages, and are often debilitating. Standard treatments, such as anti-inflammatory drugs, rehabilitation, ...

A Minimally Invasive Model to Analyze Endochondral Fracture Healing in Mice Under Standardized Biomechanical Conditions

Bone healing models are necessary to analyze the complex mechanisms of fracture healing to improve clinical fracture treatment. During the last decade, an increased use of mouse models in orthopedic research was noted, most probably because mouse models offer a large number of genetically-modified strains and special antibodies for the analysis of molecular mechanisms of fracture healing. To control the biomechanical conditions, well-characterized osteosynthesis techniques are mandatory, also in mice. Here, we report on the design and use of a closed bone healing model to stabilize femur fractures in mice. The intramedullary screw, made of medical-grade stainless steel, provides through fracture compression an axial and rotational stability compared to the mostly used simple intramedullary pins, which show a complete lack of axial and rotational stability. The stability achieved by the intramedullary screw allows the analysis of endochondral healing. A large amount of callus tissue, received after stabilization with the screw, offers ideal conditions to harvest tissue for biochemical and molecular analyses. A further advantage of the use of the screw is the fact that the screw can be inserted into the femur with a minimally invasive technique without inducing damage to the soft tissue. In conclusion, the screw is a unique implant that can ideally be used in closed fracture healing models offering standardized biomechanical conditions.

This protocol describes a minimally invasive osteosynthesis technique using an intramedullary screw for standardized stabilization of femur fractures, which can be used to analyze endochondral bone healing in mice.

Bone healing models are necessary to analyze the complex mechanisms of fracture healing to improve clinical fracture treatment. During the last decade, an ...

Using a Knee Arthrometer to Evaluate Tissue-specific Contributions to Knee Flexion Contracture in the Rat

Normal knee range of motion (ROM) is critical to well-being and allows one to perform basic activities such as walking, climbing stairs and sitting. Lost ROM is called a joint contracture and results in increased morbidity. Due to the difficulty of reversing established knee contractures, early detection is important, and hence, knowing risk factors for their development is essential. The rat represents a good model with which the effect of an intervention can be studied due to the similarity of rat knee anatomy to that of humans, the rat's ability to tolerate long durations of knee immobilization in flexion, and because mechanical data can be correlated with histologic and biochemical analysis of knee tissue.
Using an automated arthrometer, we demonstrate a validated, precise, reproducible, user-independent method of measuring the extension ROM of the rat knee joint at specific torques. This arthrometer can be used to determine the effects of interventions on knee joint ROM in the rat.

The goal of the protocol is to measure the extension range of motion of the rat knee. The effects of various diseases that increase the stiffness of the knee joint and the effectiveness of treatments can be quantified.

Normal knee range of motion (ROM) is critical to well-being and allows one to perform basic activities such as walking, climbing stairs and sitting. Lost ...

Principles and Protocols of Mechanical Testing for Bone Fracture Susceptibility

Practical Considerations for the Design, Execution, and Interpretation of Studies Involving Whole-Bone Bending Tests of Rodent Bones

Skeletal fragility leading to fracture is an American public health crisis resulting in 1.5 million fractures each year and $18 billion in direct care costs. The ability to understand the mechanisms underlying bone disease and the response to treatment is not only desired, but critical. Mechanical testing of bone serves as a valuable technique for understanding and quantifying a bone&#39;s susceptibility to fracture. While this method appears simple to perform, inappropriate and inaccurate conclusions may be reached if governing assumptions and key steps are disregarded by the user. This has been observed across disciplines as studies continue to be published with misuse of methods and incorrect interpretation of results. This protocol will serve as a primer for the principles associated with mechanical testing along with the application of these techniques-from considerations of sample size through tissue harvesting and storage, to data analysis and interpretation. With this in hand, valuable information regarding a bone&#39;s susceptibility to fracture may be obtained, furthering understanding for both academic research and clinical solutions.

Author Spotlight: Enhancing Accuracy and Reproducibility in Whole Bone Bending Tests 

Mechanical testing of rodent bones is a valuable method for extracting information regarding a bone's susceptibility to fracture. Lacking proper practical understanding, the results may be overinterpreted or lack validity. This protocol will serve as a guide to ensure mechanical tests are performed accurately to provide valid and functional data.

Skeletal fragility leading to fracture is an American public health crisis resulting in 1.5 million fractures each year and $18 billion in direct care ...

A Morphometric and Cellular Analysis Method for the Murine Mandibular Condyle

The temporomandibular joint (TMJ) has the capacity to adapt to external stimuli, and loading changes can affect the position of condyles, as well as the structural and cellular components of the mandibular condylar cartilage (MCC). This manuscript describes methods for analyzing these changes and a method for altering the loading of the TMJ in mice (i.e., compressive static TMJ loading). The structural evaluation illustrated here is a simple morphometric approach that uses the Digimizer software and is performed in radiographs of small bones. In addition, the analysis of cellular changes leading to alterations in collagen expression, bone remodeling, cell division, and proteoglycan distribution in the MCC is described. The quantification of these changes in histological sections - by counting the positive fluorescent pixels using image software and measuring the distance mapping and stained area with Digimizer - is also demonstrated. The methods shown here are not limited to the murine TMJ, but could be used on additional bones of small experimental animals and in other regions of endochondral ossification.

This manuscript presents methods for analyzing morphometric and cellular changes within the mandibular condyle of rodents.

The temporomandibular joint (TMJ) has the capacity to adapt to external stimuli, and loading changes can affect the position of condyles, as well as the ...

Biology

Transverse Fracture of the Mouse Femur with Stabilizing Pin

Fracture repair is an essential function of the skeleton that cannot be reliably modeled in vitro. A mouse injury model is an efficient approach to test whether a gene, gene product or drug influences bone repair because murine bones recapitulate the stages observed during human fracture healing. When a mouse or human breaks a bone, an inflammatory response is initiated, and the periosteum, a stem cell niche surrounding the bone itself, is activated and expands. Cells residing in the periosteum then differentiate to form a vascularized soft callus. The transition from the soft callus to a hard callus occurs as the recruited skeletal progenitor cells differentiate into mineralizing cells, and the bridging of the fractured ends results in the bone union. The mineralized callus then undergoes remodeling to restore the original shape and structure of the healed bone. Fracture healing has been studied in mice using various injury models. Still, the best way to recapitulate this entire biological process is to break through the cross-section of a long bone that encompasses both cortices. This protocol describes how a stabilized, transverse femur fracture can be safely performed to assess healing in adult mice. A surgical protocol including detailed harvesting and imaging techniques to characterize the different stages of fracture healing is also provided.

This protocol describes a method to perform fractures on adult mice and monitor the healing process.

Fracture repair is an essential function of the skeleton that cannot be reliably modeled in vitro. A mouse injury model is an efficient approach to test ...

Establishing a Diaphyseal Femur Fracture Model in Mice

Bones have a significant regenerative capacity. However, fracture healing is a complex process, and depending on the severity of the lesions and the age and overall health status of the patient, failures can occur, leading to delayed union or nonunion. Due to the increasing number of fractures resulting from high-energy trauma and aging, the development of innovative therapeutic strategies to improve bone repair based on the combination of skeletal/mesenchymal stem/stromal cells and biomimetic biomaterials is urgently needed. To this end, the use of reliable animal models is fundamental to better understanding the key cellular and molecular mechanisms that determine the healing outcomes. Of all the models, the mouse is the preferred research model because it offers a wide variety of transgenic strains and reagents for experimental analysis. However, the establishment of fractures in mice may be technically challenging due to their small size. Therefore, this article aims to demonstrate the procedures for the surgical establishment of a diaphyseal femur fracture in mice, which is stabilized with an intramedullary wire and resembles the most common bone repair process, through cartilaginous callus formation.

This protocol describes a surgical procedure for the establishment of a diaphyseal fracture in the femur of mice, which is stabilized with an intramedullary wire, for fracture healing studies.

Bones have a significant regenerative capacity. However, fracture healing is a complex process, and depending on the severity of the lesions and the age ...

3D Visualization of Bone Remodeling Under Tensile Load in Suture Expansion Mice

A 3-D Visualization Technique for Bone Remodeling in a Suture Expansion Mouse Model

Craniofacial sutures play a crucial role beyond being fibrous joints connecting craniofacial bones; they also serve as the primary niche for calvarial and facial bone growth, housing mesenchymal stem cells and osteoprogenitors. As most craniofacial bones develop through intramembranous ossification, the sutures' marginal regions act as initiation points. Due to this significance, these sutures have become intriguing targets in orthopedic therapies like spring-assisted cranial vault expansion, rapid maxillary expansion, and maxillary protraction. Under orthopedic tracing force, suture stem cells are rapidly activated, becoming a dynamic source for bone remodeling during expansion. Despite their importance, the physiological changes during bone remodeling periods remain poorly understood. Traditional sectioning methods, primarily in the sagittal direction, do not capture the comprehensive changes occurring throughout the entire suture. This study established a standard mouse model for sagittal suture expansion. To fully visualize bone remodeling changes post-suture expansion, the PEGASOS tissue clearing method was combined with whole-mount EdU staining and calcium chelating double labeling. This allowed the visualization of highly proliferating cells and new bone formation across the entire calvarial bones following expansion. This protocol offers a standardized suture expansion mouse model and a 3-D visualization method, shedding light on the mechanobiological changes in sutures and bone remodeling under tensile force loading.

Author Spotlight: PEGASOS Tissue Clearing Technique to Visualize Bone Remodeling 

This protocol presents a standardized suture expansion mouse model and a 3-D visualization method to study the mechanobiological changes of the suture and bone remodeling under tensile force loading.

Craniofacial sutures play a crucial role beyond being fibrous joints connecting craniofacial bones; they also serve as the primary niche for calvarial and ...

Cantilever Bending of Murine Femoral Necks

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