Quantification of Atherosclerosis in Mice

Summary

Murine models of atherosclerosis are useful tools to investigate pathogenic pathways on a molecular level, but require standardized quantification of lesion development. This protocol describes an optimized method to determine lesion size in the major arterial vessels including the aortic root, aortic arch, and brachiocephalic artery.

Abstract

Cardiovascular disease is the main cause of death in the world. The underlying cause in most cases is atherosclerosis, which is in part a chronic inflammatory disease. Experimental atherosclerosis studies have elucidated the role of cholesterol and inflammation in the disease process. This has led to successful clinical trials with pharmaceutical agents that reduce clinical manifestations of atherosclerosis. Careful and well-controlled experiments in mouse models of the disease could further elucidate the pathogenesis of the disease, which is not fully understood. Standardized lesion analysis is important to reduce experimental variability and increase reproducibility. Determining lesion size in aortic root, aortic arch, and brachiocephalic artery are common endpoints in experimental atherosclerosis. This protocol provides a technical description for evaluation of atherosclerosis at all these sites in a single mouse. The protocol is particularly useful when material is limited, as is frequently the case when genetically modified animals are being characterized.

Introduction

Cardiovascular disease is the main cause of death in the world with ischemic heart disease and stroke accounting for one in every four deaths¹. Most cases are caused by atherosclerosis, a disease characterized by a slow build-up of lipid-laden plaques with signs of chronic inflammation in large- and medium-sized arteries². The disease usually remains unnoticed over several decades until a rupture or erosion of the plaque elicits an arterial thrombosis that leads to ischemic tissue damage.

A normal artery consists of an intima layer with endothelial cells and sparsely distributed smooth muscle cells, a media layer with smooth muscle cells and elastic lamellae, and a surrounding adventitial layer with loose connective tissue³. An intimal retention of LDL offsets atherosclerosis development⁴. Accumulation and modification of lipoproteins lead to aggregation and entrapment within the arterial intima⁵. An inflammatory response is evoked by the trapped and modified lipoproteins⁶. Endothelial cells start to express adhesion molecules, such as VCAM-1 at sites in the arterial tree with turbulent blood flow, leading to recruitment of circulating monocytes and other leukocytes⁷. The infiltrating monocytes differentiate into macrophages that engulf lipid with ensuing transformation to macrophage foam cells⁸.

Atherosclerosis has been studied in mouse models with increasing frequency since the mid-1980s. C57BL/6 is the most commonly used inbred mouse strain for these studies, and it is used as the genetic background for the majority of genetically modified strains⁹. This strain was established in the 1920’s¹⁰, and its genome was published in 2002¹¹. Experiments in mouse models have several benefits: the colonies reproduce fast, housing is space-efficient, and inbreeding reduces experimental variability. The model also allows for genetic manipulations, such as targeted gene deletions and insertion of transgenes. This has led to new pathophysiological understanding of the disease and new therapy targets¹².

Wild-type C57BL/6 mice are naturally resistant to atherosclerosis. They have most of the circulating cholesterol in HDL, and complex atherosclerotic lesions are not formed even when fed a high-fat and high-cholesterol diet¹³. Hypercholesterolemic mice, such as Apoe^-/- on the C57BL/6-background, are therefore used as experimental models of atherosclerosis^14,15. The lack of ApoE impairs hepatic uptake of remnant lipoproteins and severely perturbs lipid metabolism. In Apoe^-/- mice, circulating cholesterol is predominantly in VLDL particles, and the mice develop complex atherosclerotic plaques on a regular chow diet.

Ldlr^-/- mice mimic the development of atherosclerosis seen in humans with familial hypercholesterolemia¹⁶. The Ldlr^-/- mice need a Western type diet to develop atherosclerosis¹⁷. Western diet mimics human food intake and usually contains 0.15% cholesterol. The LDL receptor recognizes ApoB100 and ApoE and mediates uptake of LDL particles through endocytosis. LDL receptors are fundamental for liver clearance of LDL from circulation, while LDL receptor expression in hematopoietic cells does not influence this process. This opens the possibility for bone marrow transplantation of Ldlr^+/+ cells into hypercholesterolemic Ldlr^-/- recipients and assessment of atherosclerosis development. Bone marrow chimeras have commonly been used to study the participation of hematopoietic cells in experimental atherosclerosis. However, bone marrow transplantation could influence the size and composition of atherosclerotic plaques, making interpretation of results ambiguous.

Different variants of Apoe^-/- and Ldlr^-/- mice with additional genetic alterations have been developed to study specific processes of the disease¹⁸. One example is human APOB100-transgenic Ldlr^-/- (HuBL) mice that carry the full-length human APOB100 gene^19,20. These mice develop hypercholesterolemia and atherosclerosis on a regular chow diet. However, the development of complex atherosclerotic plaques takes at least six months and shorter experimental protocols usually use Western diet²¹. A large fraction of plasma cholesterol is circulating in LDL particles, which gives HuBL mice a more human-like dyslipidemic lipoprotein profile compared to Apoe^-/- and Ldlr^-/- mice. HuBL mice also allow studies of human apoB as an autoantigen²².

The mouse models of atherosclerosis develop complex atherosclerotic plaques with shared features of human disease. However, the plaques are fairly resistant to rupture with ensuing myocardial infarction. Atherothrombosis is only sporadically detected and experimentally challenging to assess^23,24,25. Special models of plaque rupture have been developed, but the experimental field lacks a reliable and reproducible model for assessment of plaque stabilizing agents.

Quantification of atherosclerosis has been reported in numerous ways in the literature. Recent efforts have tried to standardize experimental design, execution, and reporting of animal studies²⁶. Investigators have different preferences and techniques adapted to their laboratories. Most research projects are also unique in a way that they require some protocol modifications. Due to the multifactorial nature of the disease, optimal controls vary between projects. Local conditions and lack of standardization may cause observed differences in disease development, which hampers advances of the research field. Differences in experimental variability also means that statistical power calculations need to be based on pilot studies under local conditions.

Quantification of atherosclerosis is recommended at several locations in the vascular tree. This protocol describes how to obtain results from the aortic root, the aortic arch, and the brachiocephalic artery in a single mouse, in addition to leaving the rest of the thoracoabdominal aorta for other analyses. En face preparations allow rapid quantification of lipid-laden plaques in the aortic arch. Disease burden in the brachiocephalic artery can also be quantified if the specimens are carefully displayed. The more time consuming cross-sectioning of the aortic root leaves several sections available for detailed evaluation of plaque composition.

Protocol

All animal experiments require approval by ethical authorities.

1. Mouse Sacrifice and Microdissection of Aorta

1. Sacrifice the mouse by CO₂ asphyxiation and record weight.
2. Spray the mouse with 70% ethanol to avoid fur contamination of the samples. Place the mouse in a supine position. From the jugular notch, make a midline incision using Mayo scissors extending it almost down to the pubic bone.
   CAUTION: High percentage ethanol is highly flammable and could cause serious eye irritation. Take precautionary measures.
3. Use a 23 G needle to exsanguinate the mouse by cardiac puncture through the thorax wall. This procedure usually yields 750 µL of blood from a 20 week old mouse. Typically, collect half of the volume in a tri-potassium EDTA-coated tube and the other half in a serum or lithium heparin-coated tube. Gently turn the tubes and keep them at room temperature until further processing.
4. Use Mayo scissors to cut the parietal peritoneum in the midline to open the abdominal cavity. Hold the xiphoid process with tissue forceps and cut open the peritoneum laterally on both sides and continue to open the diaphragm.
   1. Use the Mayo scissors to open the chest cavity by cutting through the rib cage as laterally as possible. This will enable wide angles for the instruments while microdissecting the aorta later on.
5. Make an incision in the right auricle for perfusion fluid drainage. Insert a 27 G needle through the apex of the heart in cranial direction. Keep the needle fixed in the left ventricle while slowly perfusing the mouse with 10 mL ice-cold phosphate-buffered saline (PBS) during minimum 2 min. Observe the liver shifting in color and getting paler.
   NOTE: Some protocols use paraformaldehyde perfusion, but this interferes with several downstream applications, such as immunohistochemistry analysis of lymphocytes. Therefore, no perfusion fixation with paraformaldehyde is performed in this protocol.
6. Dissect organs of interest (e.g. lymph nodes, spleen, liver, intestine, inguinal fat pads, kidneys, etc.) using anatomical forceps and dissecting scissors.
7. Cut trachea and esophagus on the right side of the heart without damaging the aortic arch. Cut the diaphragm and structures attaching the viscera to retroperitoneum, leaving the heart, aorta, and kidneys in situ. Fold away the lungs and viscera caudally and cover them with a napkin to begin retroperitoneal microdissection of para-aortic lymph nodes and abdominal aorta.
8. Start microdissection under a stereomicroscope at 6x magnification. Begin to dissect the aortic bifurcation by lifting surrounding tissue with Dumont forceps and cutting under tension with Vannas scissors.
   1. Continue dissection of the abdominal aorta cranially. Cut abdominal branches from the aorta and free the aorta proximally through the aortic hiatus in the diaphragm.
      NOTE: Microdissection requires accurate hand-eye coordination through the stereomicroscope, which takes some practice to master.
9. Remove the adipose tissue covering the thoracic aorta. Carefully dissect dorsally of the thymus to free the aortic arch with branches. Continue dissecting the carotid arteries as distally as possible in the thoracic cavity. In special cases, neck dissection could be performed to include the carotid bifurcation.
10. Clean the instruments by consecutive rinses in deionized water, RNase decontamination solution, 70% ethanol, and PBS before actually cutting the aorta. Lift the heart by the apex with the forceps. Cut the aorta close to the heart and place the whole heart in a tube with PBS. The heart could be stored on ice for a couple of hours before continued processing and cryomounting the aortic root.
11. Cut the aortic arch according to Figure 1A. Put the aortic arch in a tube containing 1 mL of 4% formaldehyde overnight at 4 °C. The specimen could be stored in this manner for several years before pinning and analysis.
    CAUTION: Formaldehyde may cause cancer, allergic skin reactions, and is harmful if swallowed. Use personal protective equipment as required.
12. Dissect the remaining descending aorta and put it in an RNA stabilization solution or snap freeze it for subsequent RNA analysis or other application. Optimizing work flow to minimize dissection time is crucial to avoid excessive RNA degradation.
13. Put the blood collection tubes (collected in step 1.3) in a centrifuge. Spin down the separate plasma and serum tubes at 1,500 x g for 15 min at room temperature. Carefully transfer the plasma and serum to microcentrifuge tubes and store at -80 °C. Collecting both EDTA and heparinized plasma or serum leaves possibilities for multiple downstream applications.
14. Place the heart on a cork bed with the ventral side facing up. Fix the heart to the cork with a needle through the apex. Hold the base of the heart with anatomical forceps.
    1. Use a scalpel to cut away the apical 2/3 of the heart with the direction of the cut being as a line between the two auricles with the scalpel angled 20° caudally in the sagittal plane and 20° cranially in the transversal plane (Figure 1B).
15. Embed the aortic root in optimum cutting temperature (OCT) compound, which surrounds, but do not infiltrate the tissue. Immerse the base of the heart in OCT compound. Gently squeeze the heart with the forceps to fill the aortic root with OCT and remove any air bubbles.
16. Transfer the specimen to the bottom of a cryomold filled with OCT. The aortic root should now be perpendicular to the bottom surface. Put the mounted heart on dry ice to freeze. Store the specimens in zip lock bags in -80 °C until pursuing cryosectioning according to section 3 in this protocol.

Figure 1: Heart and aortic arch in situ. (A) Lungs, trachea, esophagus, and thymus are removed to display the aortic arch in situ in a 20 weeks old female Apoe^-/- mouse on regular chow diet in a micrograph, Scale bar = 2 mm. The dotted lines indicate where to cut the aortic arch and its branches. (B) A schematic depiction of the heart and aorta. The dotted line in red indicates where to cut the heart before cryomounting the aortic root. Please click here to view a larger version of this figure.

2. En Face Analysis of Aortic Arch and Brachiocephalic Artery

1. Prepare pinning beds for en face analysis of aortic arches. Fold a segment of paraffin wax film eight times to make a flat 25 mm x 25 mm surface. Wrap it with black electric insulation tape to make a dark background for the aorta. Place a label on the backside of the pinning bed and use a lead pencil to write the mouse identification number (normal pen ink will disappear in the staining process).
2. Transfer the aortic arch to the pinning bed and place a drop of PBS on top of it. Begin cleaning the aorta from remaining periadventitial adipose tissue under a stereomicroscope.
   1. Use Vannas scissors and Dumont forceps to gently peel away all surrounding adipose tissue without manipulating or damaging the aorta. The Sudan IV will stain adipose tissue brightly and it is crucial to remove all such tissue at this point.
      NOTE: Keep the aorta moist at all times applying additional PBS when needed.
3. Cut open the aorta in the coronal plane by introducing the Vannas scissors in the aortic lumen to expose the intimal surface. Begin to cut the outer curvature of the ascending arch in distal direction and continue to cut open the branches including the brachiocephalic artery. Spare the dorsal part of the descending thoracic region.
   1. Cut open the lesser curvature and fold open the aorta to display the intimal surface.
      NOTE: This step requires fine motor skills and needs some practice to master.
4. Pin the open arch to the pinning bed using the blunt end of minutien insect pins. Use a micro Castroviejo needle holder to put the pins in place. Gently bend the pins away from the specimen when in place. Pin the aorta flat on the bed without stretching the specimen. Store the pinned arch facing downwards in a Petri dish filled with PBS at 4 °C.
   NOTE: The protocol can be paused here.
5. Prepare a working solution of Sudan IV. Mix 1 g of Sudan IV powder, 100 mL of 70% ethanol, and 100 mL of acetone in a dark bottle and gently stir for 10 min. There is no need to filter the solution and it can be used for a couple of months if kept dark at room temperature. If the staining color is not satisfactory, a new solution can be made and the specimens stained again.
   CAUTION: Acetone is a flammable liquid that could cause serious eye irritation. Store in a well-ventilated place and take precautionary measures when handling.
6. Arrange five Petri dishes on the lab bench: one filled with 70% ethanol, one filled with Sudan IV working solution, two filled with 80% ethanol, and one filled with PBS.
   1. Start with rinsing the specimen in 70% ethanol for 5 min by placing the pinning bed in the first Petri dish with the arch facing downwards. Transfer the specimen to the Sudan IV working solution and let it stain the arch for 7 min.
   2. Next, rinse in 80% ethanol for 3 min twice to destain the normal intimal surface. Destaining time could be adjusted to optimize results. Lastly, rinse in PBS before putting the specimen back into the original Petri dish.
7. Acquire micrographs using a stereomicroscope at 10 times magnification connected to a digital camera. Take pictures of the pinned arch submerged in PBS using small metal weights (20 mm x 10 mm x 5 mm) to hold the pinning bed to the bottom of a Petri dish. Place a ruler next to the aorta for calibration of the image.
8. Use an image analysis software (e.g. ImageJ) to determine lesion area and total intimal surface. In lack of anatomical landmarks to define the aortic arch, measurement is usually performed from the start of the ascending aorta down to the first intercostal branch (Figure 2A). Use the area quantification feature in the software to manually encircle the total intimal arch area.
   NOTE: The lesion quantification should be done in a blinded fashion and it is advisable that a second investigator confirms the results.
   1. In ImageJ, select the polygon selection tool and encircle the total arch area by repetitive clicks. Then select measure in the analyze menu to display the total arch area in the result window.
   2. Next, encircle all Sudan IV-stained plaques in the arch. Sudan IV is a lysochrome diazo dye that stains lipids, triglycerides, and lipoproteins with an orange-red color. In ImageJ, select the freehand selection tool and encircle all plaques while pressing the Alt key. Click measure in the analyze menu to display lesion-free arch area in the result window.
   3. Calculate relative lesion area by subtracting the lesion-free area from the total arch area and then dividing the result with the total arch area.
9. Carefully pin the subclavian and carotid arteries to enable lesion quantification in the brachiocephalic artery (Figure 2A). Quantification of lesions in the subclavian arteries and the common carotid arteries is usually very challenging and not meaningful, respectively.
   1. In ImageJ, encircle both pieces of the braciocephalic artery using the polygon selection tool while pressing the shift key. Click measure in the analyze menu to display the total brachiocephalic artery area in the result window.
   2. Next, select the freehand selection tool and encircle all plaques in brachiocephalic artery while pressing the Alt key. Click measure in the analyze menu to display the lesion-free brachiocephalic artery area in the result window.
   3. Calculate relative lesion area by subtracting the lesion-free area from the total brachiocephalic artery area and then dividing the result with the total brachiocephalic artery area.

Figure 2: Atherosclerotic lesion quantification. (A) Aortic arch from a 20 weeks old male human APOB100-transgenic Ldlr^-/- (HuBL) mouse fed Western diet for ten weeks pinned open and stained for lipid-rich plaques with Sudan IV. Total aortic arch surface area is outlined with the dotted line in white in the micrograph, Scale bar = 2 mm. The dotted lines in yellow outline the total surface area of the brachiocephalic artery. (B) Aortic root cross-section at 400 µm from the aortic sinus in a 20 weeks old male Ldlr^-/- mouse fed Western diet for eight weeks visualized in a micrograph, Scale Bar = 500 µm. The dotted lines in black outline the total vessel area and atherosclerotic lesions stained with Oil Red O localized in the arterial intima. Please click here to view a larger version of this figure.

3. Cryosectioning of the Aortic Root

1. Set the cryostat temperature at -20 °C and section thickness to 10 µm. Mount the OCT block containing the aortic root on the specimen holder with the ventricular tissue facing outward. While starting to cut, fine tune the alignment of the section surface to be parallel to the specimen holder.
2. Remove excessive surrounding OCT to make it easier to collect sections without folds. The aortic root should now be positioned perpendicular to the knife blade given that the base of the heart was placed correctly in the mold.
3. Collect initial control sections on ordinary microscope slides, which will be discarded. The first sections should only contain heart muscle tissue. Progress the sectioning by 200 µm at the time. Collect a section and check the progress with a light microscope.
4. When getting closer to the left ventricle outflow tract, check every 100 µm under the microscope. When initial indications of a vessel wall are observed, slow down the pace to 50 µm.
   NOTE: When the first aortic cusp appears, this will be point zero for collecting sections. It can be difficult to see when the cusps appear exactly, but an exact localization is crucial to perform comparisons of lesions in the same region.
5. Tilt the specimen towards the point zero cusp to align the section plane with the two other cusps. This is crucial for obtaining true cross sections of the aorta. Make a drawing of the aortic root, indicating the cusps as they appear, and count every 10 µm section that are cut from point zero onwards.
   1. When a second cusp appears, slightly tilt the specimen again away from the cusp to align the specimen with the third cusp. The level difference between the cusps should not exceed 50 µm. Start to collect sections on slides from level 90 µm and onwards.
   2. Collect sections according to the slide planning in Figure 3. The collection of sections may be started from 190 µm if the aortic root is more than 50 µm tilted, to allow further space to align the root in a straight position. Continue sectioning until reaching level 800 µm from point zero. If there are still visible plaques at this level, the collection could be expanded to 1,000 µm.
      NOTE: A simplified slide organization is presented in Supplemental Figure 1, which could increase sectioning speed. The optimal slide planning should be decided depending on the project plan.
6. Fix the sections after collection.
   1. Fix the sections collected for Oil Red O staining and Picrosirius red staining of collagen in 4% formaldehyde for 10 min. Rinse in deionized water, dry, and store in room temperature until pursuing with section 4 in this protocol. If slides should be stained with Oil Red O right away and are still wet, place them in 60% isopropanol for 1 min to speed up the drying process.
      CAUTION: Isopropanol is a flammable liquid that could cause serious eye irritation and may cause drowsiness or dizziness. Store in a well-ventilated place and take precautionary measures when handling.
   2. Fixate the sections collected for immunohistochemistry or immunofluorescence in ice cold pure acetone for 10 min. Dry in room temperature for 30 min. Store sections in -20 °C.

Figure 3: Organization of slides for serial sections of the aortic root. During cryosectioning of the aortic root every 10 µm thick section spanning the first 800 µm of the ascending aorta should be collected. A systematic slide organization is needed to obtain suitable sections for various applications. Analysis of lesion composition usually includes Oil Red O staining for lipids and Picrosirius red staining for collagen. Remaining sections are collected and acetone-fixed for immunohistochemistry and immunofluorescence staining. This figure has been modified from Gisterå et al³⁰. Please click here to view a larger version of this figure.

4. Oil Red O Staining and Quantification of Atherosclerosis in Aortic Roots

1. Prepare a saturated Oil Red O solution by dissolving 1 g of Oil Red O in 100 mL of isopropanol. Stir the solution in a dark bottle for 1 hour at room temperature. The saturated solution can be kept for several months.
   NOTE: It is advisable to have designated laboratory equipment for Oil Red O staining since it is difficult to clean equipment that has been in contact with the solution.
2. Prepare a working solution by mixing 75 mL of the saturated Oil Red O solution with 50 mL of deionized water. Let stand in room temperature for 10 min. Filter through a qualitative filter paper.
3. Place the slides in Oil Red O working solution for 20 min. Rinse in tap water for 5 min.
4. To assist tissue visualization, stain with Mayer’s hematoxylin for 1 min. Rinse in lukewarm tap water for 5 min. All nuclei should now be stained in blue color, adjust staining time to optimize the result.
5. Mount slides in an aqueous mounting medium (e.g., Kaiser’s glycerol gelatin). Warm Kaiser’s glycerol gelatin to 40 °C to make it fluid before use. It is not necessary to dry the slides since the mounting medium is water based. Be careful to avoid air bubble formation when adding the cover glass.
   CAUTION: Kaiser’s glycerol gelatin contains phenol, which is suspected of causing genetic defects. Use personal protective equipment as required.
6. Acquire digital micrographs using a camera connected to a light microscope. Usually the full vessel wall and lesion boundaries could be clearly visualized by 50 times magnification. Save high resolution images, preferably in tagged image file format (TIFF).
7. Perform analysis of lesion size using a computer-assisted image analysis software system. Oil Red O is a lysochrome diazo dye that stains neutral lipids and visualizes atherosclerotic plaques with an intense red color, which assists lesion quantification.
   NOTE: The lesion quantification should be done in a blinded fashion and it is advisable that a second investigator confirms the obtained results.
   1. Use the area quantification feature in the image analysis software to define the total vessel area by encircling the external elastic lamina of the aortic vessel wall (Figure 2B). In ImageJ, select the polygon selection tool and encircle the area by repetitive clicks. Then select measure in the analyze menu. The total vessel area is displayed in the result window.
   2. Continue to quantify the atherosclerotic lesions in the intimal layer of the vessel, defined by the internal elastic lamina and the luminal boundary. Usually lesions on valve cusps are excluded from the measurement²⁷. In ImageJ, select the freehand selection tool and encircle all plaques while pressing the Alt key. Select measure in the analyze menu to display the lesion-free vessel area in the result window.
   3. Calculate the relative lesion area by subtracting the lesion-free area from the total vessel area and then dividing the result with the total vessel area.
      NOTE: Calibrate the results in the image analysis software according to the used magnification to obtain absolute lesion area in square micrometer.
8. Define the Oil Red O-stained area in the lesions by using a color threshold feature in the image analysis software to calculate the percentage of Oil Red O positive area of total lesion area.
   1. In ImageJ, encircle all lesion area by using the freehand selection tool while pressing the shift key. Select measure in the analyze menu to display total lesion area is in the result window.
   2. Select clear outside in the edit menu. Change the image type to 8-bit in the image menu.
   3. Set a red threshold for Oil Red O negative area by selecting threshold in the adjust submenu of the image menu. Click apply. Make the image binary by selecting this option in the binary submenu of the process menu.
      NOTE: Usually Oil Red O staining varies between batches. Hence, color thresholding is only recommended within the same staining batch. The result should be presented along with a description how the threshold was determined and standardized.
   4. Analyze the picture by selecting analyze particles in the analyze menu and click ok. Total Oil Red O negative lesion area is now displayed in the summary window. Calculate the relative Oil Red O positive area by subtracting the Oil Red O negative area from the total lesion area and then dividing with the total lesion area.

Discussion

Cardiovascular disease is the main killer in the world and new preventive measurements are needed². Mouse models of the disease provide a comprehensive platform for investigation of pathophysiology and experimental treatments¹³. Reliable lesion size quantification is essential for this approach. However, quantification methods differ between laboratories. Standardization and optimization have been an ongoing process since the 1980’s^13,27,33,34. Aortic roots have emerged as the most popular site to quantify experimental atherosclerosis. Cross-sections of plaques enable comparison of plaque volume between groups. En face preparations are favored for lesion quantification in larger segments of the aorta. The en face method visualizes plaque quantity and enables quantification of plaque area coverage, but do not take plaque thickness in account. The biological relevance for observed differences is substantiated by coherent results at different locations in the vascular tree. Evaluating atherosclerosis development at different locations addresses possible site specific effects. The effect of transplanted hematopoietic cells on atherosclerosis development can be assessed in hypercholesterolemic Ldlr^-/- chimeras. However, whole-body irradiation affects the atherosclerosis process with site specific effects. More prominent atherosclerotic lesions are developed in the aortic root, while reduced lesion development is observed in aortic arches³⁵.

Importantly, not only lesion size needs to be addressed in studies of experimental atherosclerosis. Lesion composition is also a key parameter. Several plaque features have been associated with manifestations of the disease in humans³⁶. Serial sectioning of the aortic root leaves several sections available for careful analysis of plaque composition. Plaque rupture in humans is characterized by a thin fibrous cap with few smooth muscle cells, sparse collagen content and signs of inflammation in the plaques³⁶. Although plaque rupture is a rare event in mouse models of atherosclerosis, markers for plaque stability are informative to evaluate. Translational approaches could confirm mechanistic findings from mouse models and uncover important features of human disease³¹. Inflammatory status of atherosclerotic plaques could be determined by immunohistochemistry staining of VCAM-1, MHC class II, macrophages, and lymphocytes³⁰. Some protocols use longitudinal sections in the coronal plane of the aortic arch or the brachiocephalic artery for measuring atherosclerotic lesion size and composition³⁷. However, this alternative method leaves only few sections to be analyzed, which limits its applications.

An initial critical step in this protocol is the ability to harvest aortas efficiently. Hand-eye coordination under the microscope requires practice and is crucial both for the microdissection and the subsequent pinning of the aortic arch. The next critical step in this protocol is the collection of serial sections from the aortic root. Eighty consecutive sections should be collected for each mouse, which requires both focus and patience. Methodological proficiency could speed up the described processes considerably. Nevertheless, atherosclerotic lesion quantification is still a time-consuming task. New technology, automated handling, and small animal imaging might facilitate quantification of experimental atherosclerosis in the future. The progression of atherosclerosis is slow and most experimental protocols in mouse models take more than four months to complete¹³. Therefore, aortas need to be collected in an optimized way at study endpoints. This protocol provides a comprehensive guide to harvest aortas efficiently and the proposed processing prepares aortas for multi-purpose use including lesion quantification in aortic root, aortic arch, and brachiocephalic artery. Hopefully the protocol can reduce experimental variability, enhance reliability of results, and lead to findings that will pave the way for new treatments against atherosclerosis.

Materials

Name	Company	Catalog Number	Comments
Acetone	VWR Chemicals	20066.296	For fixation of sections for immunohistochemistry.
Black electrical insulation tape (50 mm wide)	Any specialized retailer	-	To create pinning beds for aortic arches.
Centrifuge	Eppendorf	5417C	Benchtop microcentrifuge.
Cork board	Any specialized retailer	-	For cutting hearts in the preparation to cryomount aortic roots.
Cryostat	Thermo Scientific	Microm HM 560	For serial cryosectioning of aortic roots.
Deionized water	-	-	For rinsing and preparation of solutions.
Digital camera	Leica Microsystems	DC480	5.1 megapixel CCD for high-resolution images of aortic arches and aortic root sections.
Dissecting scissors (10 cm, straight)	World Precision Instruments	14393	For general dissection of organs.
Dumont forceps #5 (11 cm, straight)	World Precision Instruments	500341	For microdissection of aorta.
Ethanol 70% (v/v)	VWR Chemicals	83801.290	Highly flammable liquid and vapour, store in a well-ventilated place, and keep cool.
Ethanol absolute ≥99.8%	VWR Chemicals	20821.310	Highly flammable liquid and vapour, store in a well-ventilated place, and keep cool.
Formaldehyde 4% stabilised, buffered (pH 7.0)	VWR Chemicals	9713.1000	Harmful by inhalation, in contact with skin and if swallowed.
ImageJ	NIH	-	Image analysis software.
Iris forceps (10 cm, curved, serrated)	World Precision Instruments	15915-G	Used as anatomical forceps.
Isopropanol	Merck	1096341011	Flammable liquid, causes serious eye irritation, and may cause drowsiness or dizziness.
Kaiser's glycerol gelatine	Merck	1092420100	Aqueous mounting medium containing phenol. Suspected of causing genetic defects.
Light microscope	Leica Microsystems	DM LB2	For analysis during sectioning and documentation of Oil Red O stained micrographs.
Mayer's hematoxylin	Histolab	1820	Non-toxic staining solution without chloral hydrate, but causes serious eye irritation.
Mayo scissors (17 cm, straight)	World Precision Instruments	501751-G	For general dissection.
Micro Castroviejo needle holder (9 cm, straight)	World Precision Instruments	503376	For pinning of aortic arches.
Microcentrifuge tubes	Corning	MCT-175-C	Polypropylene microtubes with snaplock cap.
Microlance 3 needles, 23 gauge	BD	300800	For blood collection.
Microlance 3 needles, 27 gauge	BD	302200	For perfusion of mice.
Microvette 500 µL, K3 EDTA	Sarstedt	20.1341.100	For blood collection.
Microvette 500 µL, Lithium Heparin	Sarstedt	20.1345.100	For blood collection.
Minutien insect pins, 0.10 mm	Fine Science Tools	26002-10	For pinning of aortic arches.
Oil Red O	Sigma-Aldrich	O0625	Not classified as a hazardous substance or mixture.
Optimum cutting temperature (OCT) cryomount	Histolab	45830	For embedding tissue.
Parafilm M	Bemis	PM992	Paraffin wax film used to create pinning beds for aortic arches.
Petri dishes (100x20 mm)	Any cell culture supplier	-	Proposed as a storage container for pinned aortas.
Phosphate buffered saline (PBS)	-	-	Sterile and RNase-free solution is required for perfusion of mice.
Qualitative filter paper (grade 1001)	Munktell	120006	For filtering Oil Red O working solution (typical retention 2-3 µm).
RNAlater RNA stabilization reagent	Qiagen	76106	For stabilization of RNA in tissue samples
RNaseZap RNase Decontamination Solution	Invitrogen	AM9780	A surface decontamination solution that destroys RNases on contact.
Scalpel handle #3 (13 cm)	World Precision Instruments	500236	For cutting hearts in the preparation to cryomount aortic roots.
Standard scalpel blade #10	World Precision Instruments	500239	For cutting hearts in the preparation to cryomount aortic roots.
Stereomicroscope	Leica Microsystems	MZ6	For dissection and en face documentation
Sudan IV	Sigma-Aldrich	S4261	Not classified as a hazardous substance or mixture.
Superfrost Plus microscope slides	Thermo Scientific	J1800AMNZ	To collect aortic root sections.
Tissue forceps (15 cm)	World Precision Instruments	501741-G	For general dissection.
Tissue-Tek cryomolds (10x10x5 mm)	Sakura	4565	For embedding aortic roots in OCT.
Vannas scissors (8 cm, straight)	World Precision Instruments	503378	For microdissection of aorta.