Digital Planimetry for Assessing Wound Closure Kinetics in a Mouse Model

Summary

Wounds represent a global health challenge. This study developed a standardized photo booth utilizing digital planimetry to minimize wound measurement variability. Monitoring wounds in mice over 14 days revealed an initial increase in wound area and perimeter, followed by gradual closure. This methodology may aid in evaluating wound closure kinetics in pre-clinical models.

Abstract

Chronic wounds, due to their high prevalence, are a serious global health concern. Effective therapeutic strategies can significantly accelerate healing, thereby reducing the risk of complications and alleviating the economic burden on healthcare systems. Although numerous experimental studies have investigated wound healing, most rely on qualitative observations or quantitative direct measurements. The objective of this study was to standardize an indirect wound measurement method using digital planimetry, incorporating digital scaling and segmentation. This approach addresses the lack of detailed, step-by-step methodologies for accurate wound assessment. A photodocumentation booth was designed and constructed, and computer-assisted digital planimetry tools were employed to minimize variability in measurements of the wound area, perimeter, and the distance from the wound center to its edges. A circular traumatic wound (5 mm in diameter) was created on the dorsal midline at the shoulder blade level of male CD1 mice (n = 4, 10 weeks old, 30-35 g). Wound evolution was photodocumented for 14 days using the custom-designed photo booth, which controlled lighting conditions, focal distance, and subject positioning. Scaling and wound measurements were performed using segmentation in ImageJ software, and statistical analysis was conducted using statistical analysis software. The kinetics of wound closure showed a slight increase in wound size and perimeter between day 0 and day 2, followed by a gradual decrease until complete closure by day 14. The photodocumentation booth and computer-assisted digital planimetry enabled quantitative measurements with minimal variability. In conclusion, these tools provide a reliable and reproducible method for evaluating wound closure kinetics in pre-clinical models.

Introduction

Traumatic wound healing takes approximately 21 days and has a well-defined sequence of four distinct phases: (1) hemostasis, (2) inflammation, (3) proliferation, and (4) remodelling¹. If any phase of wound healing is prolonged, it can lead to the development of chronic wounds¹. Due to their high prevalence, potential complications², and significant economic burden, they are considered a global health problem.

Pre-clinical studies aim to achieve faster healing by promoting comprehensive wound re-epithelialization^3,4,5, preventing complications, and reducing treatment costs. These studies evaluate various strategies, including the development of biomaterials, pharmacological interventions, and other regenerative medicine procedures^6,7,8,9.

Multiple experimental models have been developed for the study of traumatic wounds. Some focus on macroscopically visible qualitative characteristics such as size, inflammation indicators, presence of granulation tissue, secretions, and scab formation⁵. Others analyze quantitative data, including area, perimeter, radius, diameter, color, depth, and distances from the center to the edges of wounds.

In this regard, most in vivo investigations directly measure wound radius and depth. However, manual delineation of wound edges in a macroscopic image can introduce biases in the measurement¹⁰. Other studies use mechanical planimetry, using transparent gridded plastic sheets, where the wound edges are previously delineated; in both cases, obtaining the area or perimeter requires manual instruments such as rulers or digital planimeters. Nowadays, computer-assisted digital planimetry allows computerized analysis of macroscopic images of wounds or plastic sheets. In situ manipulation and quality of macroscopic image are a limitation, however, this tool^11,12,13,14 considerably reduces the variability between area and perimeter measurements.

This proposed methodology offers significant advantages over existing techniques for evaluating wound closure in mice^{15,16,17,18,19,20}. While photo documentation has been considered an accurate and consistent tool for assessing wound closure kinetics, previous studies^21,22 have highlighted the limitations of manual wound measurement, such as observer bias and variability due to inconsistent lighting and camera positioning. The current approach addresses these issues by standardizing imaging conditions through a custom-built booth, improving reproducibility and precision. Furthermore, computerized digital planimetry enables more accurate quantitative assessments, enhancing the evaluation of therapeutic interventions and minimizing measurement errors, as evidenced in other studies comparing manual and digital techniques^12,22 making it particularly suited for studies of wound closure kinetics in murine models, allowing precise evaluation of treatments by maintaining strict control over image acquisition conditions.

Protocol

All experimental procedures involving laboratory mice were conducted in accordance with the ethical standards and regulations established in the Official Mexican Standard (NOM-062-ZOO-1999) for the handling and care of laboratory animals. The protocol was reviewed and approved by the Internal Committee for the Care and Use of Laboratory Animals (CICUAL) of the National Institute for Nuclear Research (ININ) under reference number CICUAL-01-23. Male CD1 mice (n = 4), 10 weeks old, with a body weight ranging from 28-32 g, were used in this study. All animals were selected to ensure uniformity in strain, age, sex, and body weight, minimizing variability in the experimental outcomes. Details of the reagents and the equipment used are listed in the Table of Materials.

1. Photo booth construction for the acquisition of macroscopic images

NOTE: Licensed SolidWorks software (version 2015) was used to design a photo booth to eliminate external lighting sources. A 40 cm × 40 cm cube was constructed using a one-inch thick white aluminum profile. The cube consisted of three sections, assembled sequentially: the roof, side walls, and floor (Figure 1A).

1. Roof construction
   NOTE: The roof was regionalized as front edge (A), rear edge (B), and side edges (C and D) to orient (Figure 1B).
   1. Fix on the inner area of the side edge of the roof (C and D) a slotted aluminum profile (designed to hold glass) 1.5 cm wide, 2.51 cm thick, and 34.9 cm long (Figure 1B).
   2. Place two 34.5 cm long x 13 cm wide rectangular aluminum plates with polyethylene in the center in the groove of each roof profile (Plate 1 and 2 in Figure 1C) to enable sliding through the groove of both profiles.
   3. Install a 20 cm RGB LED tube light with a color temperature range of 2500-9000 K (Figure 1C) at a 45° angle on the underside edge of panel 1 using double-sided tape.
   4. Mount on the roof panels 1 and 2 a 32 cm x 12 cm rectangular foam board panel with a central 7.82 cm diameter circular cut-out to allow the installation of the camera lens (Figure 1C).
2. Construction of the floor
   1. Place a 40 cm x 40 cm square piece of white foam board on top of the floor area profiles. Cut squares with a side length of 2.54 cm from each corner of the foam board (Figure 1E).
3. Construction of side walls
   1. Cut four 40 cm x 40 cm quadrangular foam board panels.
   2. Glue two panels with silicone on sides C and D to form the left and right side walls (Figure 1F).
   3. Attach hook and loop fastener strips to the aluminum profiles A and B for easy manipulation of internal photo booth elements. Additionally, attach 1 cm from the edge of a line of adhesive fasteners to two foam cardboard squares on one side, and place them on the front and rear walls (Figure 1F).
4. Construction of the reference base
   NOTE: A reference base was necessary to maintain the mouse in the prone position during anesthesia and throughout the documentation of wound evolution. 3D components were designed and fabricated using the Fused Deposition Modeling (FDM) technique with PLA material and a 3D printer^23,24.
   1. 3D print the mask with a base of 2 cm in width, length, and height and place it 11.5 cm from the edge of a pre-cut 40 cm x 28 cm white foam board rectangle to maintain the mice under inhalation anesthesia (Figure 1D, red color).
   2. 3D print the rectangular platform (9 cm long, 5 cm wide, 2.5 cm high) with four extruded areas to align the mouse dorsum during image acquisition. These areas supported the head, limbs, and abdominal region to maintain the prone position. Glue this platform to the center of the reference base (Figure 1D, green color).
   3. 3D print the ruler block (2 cm wide, 8 cm long, 2.5 cm high) and fix it 1 cm from the left side of the mouse base to place the measurement reference element needed for digital image processing (Figure 1D, blue color).
   4. Attach a 15 cm stainless steel graduated ruler to the ruler block, and install the entire reference base inside the cabin for image scaling (Figure 1D).

Figure 1: Diagram for the construction of the macroscopic image acquisition cabinet. (A) Sections of the cabin (roof, side walls, floor).(B)Orientation of the profiles forming the roof; front (A), rear (B), and sides (inner side of the profiles in red "C,D"). (C) Roof panels 1 and 2, installation of the LED light tube, camera lens plate, and floor installation. (D) Installation of the anesthesia mask (RED), mouse platform (GREEN), and rectangular platform for positioning of the measuring ruler (BLUE) on the reference base. (E) Final location for the reference base. (F) Installation of sides, front, and rear walls. Please click here to view a larger version of this figure.

2. Animal maintenance

1. Obtain authorization from the institution's bioethics committee for animal testing. Use CD1 mice (n = 4), 10 weeks old, weighing 28-32 g.
2. House the mice under standard conditions: maintain a temperature of 21 °C, 12/12 h light/dark cycles, 45% humidity, and provide ad libitum access to water and food, except during photodocumentation sessions.

3. Traumatic wound generation

1. Anesthetize the mouse using inhaled sevoflurane at a concentration of 5%, delivered with an oxygen flow rate of 1.5 L/min, using a calibrated vaporizer²⁵ (following institutionally approved protocols).
   1. Confirm the depth of anesthesia by checking for a lack of withdrawal reflex during an interdigital pinch. Apply ophthalmic ointment to the eyes to prevent dryness during anesthesia. Maintain the mice at a stable temperature of 37 °C during the surgery and recovery (20 min).
2. Place the mouse in a ventral decubitus position and depilate a 2.5 cm x 3 cm area from the cervical region caudally using surgical blades. Stretch the skin to avoid lacerations. Perform asepsis and antisepsis using several rounds of alternating povidone iodine and sterile water rinses.
3. Use a sterile 5 mm biopsy punch and apply pressure with circular movements to create a dermo-epidermal incision at the shoulder blade level. Remove the flap with serrated forceps and cut with iris-tip scissors (Figure 2A).
4. If bleeding points are present in the wound, achieve hemostasis using an electrocautery device.
5. Place a 1 cm diameter circular dermal film over the wound using Jeweler forceps to prevent contamination and contraction.
6. Perform all survival surgeries under sterile conditions. Prepare the surgical site with disinfectants like povidone-iodine. Wear sterile gloves and a mask, and maintain sterility throughout the procedure by using sterile instruments and minimizing contact with non-sterile surfaces.
   1. After surgery, place the mice in individual cages at 24 °C and monitor them until they regain normal ambulation. Ensure body temperature is controlled during and after surgery to prevent hypothermia by using external heat sources.
7. Administer analgesia by dissolving ketorolac (tablet form, 10 mg) in drinking water at a concentration of 0.025 mg/mL. This corresponds to a daily dose of 5 mg/kg for a 30 g mouse consuming approximately 6 mL of water per day. Begin administration 48 h before surgery and continue until day 4 post-wounding to ensure preemptive and sustained analgesia²⁶.
8. After surgery, monitor the animals daily for at least five consecutive days. Evaluate each mouse for body condition score, coat appearance, behavioral signs of pain or distress (e.g., reduced activity, abnormal posture), and wound condition (e.g., presence of discharge, redness, swelling, or signs of infection). Record observations in an institutional animal care log. Continue regular monitoring until day 14, when wounds in healthy rodents typically reach advanced stages of healing. Euthanize the mice by O₂ replacement in a CO₂ chamber following international standards. This marks the endpoint of the study.

4. Macroscopic image acquisition

1. Capture images of the wounds daily for 14 consecutive days to monitor the continuous kinetics of wound closure. Use a semi-professional or professional camera; position the lens through the circular opening in the photo booth roof.
   NOTE: Adjust the schedule as necessary based on experimental conditions.
2. Use an RGB LED light tube in Correlated Colour Temperature (CCT) mode, set to 9000 K and 100% brightness for lighting.
3. Position the reference base at the center of the photo booth floor.
4. Place the mouse in the inhaled anesthesia chamber for 3 min (Figure 2B).
5. After inducing anesthesia, place the mouse in a prone position on the mouse platform. Secure the snout within the sevoflurane anesthesia mask, delivering 5% sevoflurane at an oxygen flow rate of 1.5 L/min (Figure 2C).
6. Before capturing images, remove the dermal film from the wound using Jeweller forceps and align the reference base with the camera lens.
7. Install the front wall of the photo booth, and capture macroscopic images with the following settings: aperture f/3.2, exposure time 1/200s, ISO speed 80, focal length 4mm.
8. Using Jeweller forceps, place a 1 cm diameter dermal film on the wound before removing the anesthesia mask. Transfer the mice to individual cages and observe until motor recovery.

5. Image processing

1. Generate a backup copy of the macroscopic images. Process the images using the ImageJ software.
2. Open the backup image in ImageJ by following the path: File > Open > Search in the images, then click on Open.
3. Scale the image by reference: Maximize the image, select the straight-line tool, zoom in on the ruler next to the mouse using the + key, draw a 10 mm straight line on the ruler image, then go to Analyze > Set Scale > Enter " 10" for Known distance > Set Unit of length to mm, and then click on Ok. This determines the pixels-to-distance ratio for the macroscopic image (Figure 2D).
4. Separate the wound area from the image: Use the rectangle tool to select the area around the wound (w = 150, h = 150). Record the X and Y values, right-click on the rectangle > Duplicate > Name the subject > Press Enter. In the new image, press + twice to zoom in (Figure 2E).
5. Save the cropped image by following the path: File > Save As > Tiff > Enter the name > Save.
6. Create a duplicate of the cropped image to avoid modification during segmentation: Right-click on the cropped image > Duplicate > Name it by adding "Segmentation" to the end. Next, press Enter. In the new image, press + twice to zoom in.
7. Separate the image into color channels by following this path: Image > Type > RGB Stack. In the red channel image (1/3 Red), right-click on Duplicate, and press OK in the Duplicate window.
8. Segment the red channel image. Click on the red channel image, Image > Adjust > Threshold. Next, select Default > Apply (Figure 2F).
9. Rectify the Region of Interest (ROI) to ensure complete wound coverage and avoid segmentation distortions.
   NOTE: If areas around the wound are not included in segmentation, go to Process > Binary > Fill Holes. To remove black dots outside the wound, go to Process > Binary > Erode. If the Erode command reduces the wound size, correct it by using Process > Binary > Dilate.
10. Mark the perimeter of the ROI: Edit > Selection > Create Selection. The ROI will be outlined in yellow. Add it to the ROI Manager by following Edit > Selection > Add to Manager (Figure 2G).
11. Validate the segmentation: Open the ROI Manager window, and select the ROI to review: More > Translate. Enter the X and Y values recorded in step 4, and press OK.
    1. Maximize the original image, then select the ROI in the ROI Manager. Adjust the ROI using the arrow keys until it aligns with the wound (Figure 2H). If the ROI matches the wound, the segmentation was successful. Otherwise, repeat from step 2.
12. Once the segmentation is confirmed, obtain the wound measurements: Analyze > Measure. A results table will display the area, perimeter, and X/Y position values. Copy these values to SPSS software for documentation and statistical analysis(Figure 2I).

Figure 2: Workflow of wound measurement using digital planimetry and segmentation techniques. (A) Dermo-epidermal incision using a sterile 5 mm biopsy punch. (B) Placing the mouse in an inhaled anesthesia chamber for 3 min. (C) Photo documentation by positioning the anesthetized mouse in the photo booth and securing its snout within a sevoflurane mask. (D) Opening the obtained image in ImageJ and scaling it using the ruler as a reference. (E) Extracting the wound area using the rectangle tool. (F) Separating the image into RGB channels and processing the red channel. (G) Outlining and managing the region of interest (ROI). (H) Validating the segmentation by matching the ROI with the wound. (I) Measuring wound parameters and recording the results for statistical analysis. Please click here to view a larger version of this figure.

6. Post-procedural euthanasia

NOTE: The study concludes after 14 days, at which point the wounds in healthy rodents typically reach advanced stages of healing. At this stage, the mice were humanely euthanized following the established institutionally approved euthanasia procedure.

1. Prepare the equipment. Ensure the euthanasia chamber is clean, dry, and of appropriate size to accommodate the mice without overcrowding. Connect the chamber to a medical-grade CO₂ supply with a flow regulator.
2. Gently transfer the mice into the chamber to minimize stress. Ensure they are in a calm environment with minimal external disturbances.
3. Set the CO₂ flow rate to 30%-70% of the chamber's volume per minute, as recommended by the AVMA Guidelines for the Euthanasia of Animals. Gradually increase the CO₂ concentration to avoid inducing distress or discomfort in the mice.
4. Observe the mice closely during the procedure. Look for signs of gradual loss of consciousness, including reduced activity and breathing, followed by apnea and cardiac arrest.
5. Confirm the death once the mice are no longer breathing and show no signs of movement; wait an additional 1-2 min to ensure a complete cessation of vital functions. Verify death by confirming the absence of reflexes (e.g., corneal reflex) and cardiac activity.
6. Transfer the carcasses to designated Biological Hazardous Waste containers. Follow institutional protocols and national guidelines for the safe disposal of animal remains.
7. Record the number of animals euthanized, the date, and any relevant observations to ensure compliance with ethical and institutional standards.

Results

After scaling the images in ImageJ software, the average perimeter (Table 1) and area (Table 2) of the wounds, along with their respective standard deviations, were obtained through digital segmentation. These values were recorded from day zero to day fourteen (D0-D14).

...

Day	Perimeter (mm)
0	22.75 ± 0.8900

Discussion

In pre-clinical models, quantitatively analyzing the evolution of traumatic wounds in pre-clinical models faces challenges due to factors like wound size, localized inflammatory response³⁴, location, and/or manipulation. Direct manual³⁶ and indirect digital^11,16,37,38 planimetry methods exist for these measurements. In contrast to studies using ma...

Materials

Name	Company	Catalog Number	Comments
5 mm Biopsy Punch	MILTEX, USA	33-35	To mark the wound edges
Aluminum with polyethylene core	Alucobond,USA	Bright Silver 119	For the construction of the macroscopic Image Acquisition Booth
Camera Lens	Sony, Japan	SEL2470Z	To focus the images to photograph
Electrocautery	Bonart, USA	ART-E1	To eliminates bleeding points in the wound if present.
Hook and loop fastener strips	VELCRO
IBM SPSS Statistics Version 22	IBM Corporation, USA	https://www.ibm.com/analytics/spss-statistics	Used for statistical analysis of wound measurements, including area and perimeter data.
ImageJ Version 1.53t	National Institutes of Health, USA	https://imagej.nih.gov/ij/	Used for processing macroscopic images, including scaling, segmentation, and measurement of wound parameters.
Ketorolac	SIEGFRIED RHEIN, Mexico	493977	For postoperative pain management
Miltex Iris Scissors, 4-1/8" Curved	MILTEX, USA	V95-306	To cut the wound flap generated with the biopsy punch
RGB LED Light Tube	ANDOER, China	‎ B09F8RLMSY	To illuminate the Macroscopic Image Acquisition Booth
Semi profesional camera	Sony, Japan	DSC-HX300	To take the photos
Serrated Forceps	MILTEX, USA	V96-118	To hold the flap during the cut
Sevoflurane	Baxter, USA	AMX2L9117PR	For inhaled anaesthesia
Sodium Pentobarbital	Aranda, Mexico	734.448.001.212	For intraperitoneal anaesthesia
SolidWorks Version 2015	Dassault Systèmes, France	https://www.solidworks.com/	Used to design and create 3D models for constructing  accessories for the photodocumentation booth.
Surgical blades	HERGOM, Mexico	H10	To shave the hair in the area where the wound will be created
Transparent Adhesive Dressing	3M, USA	F51CA07	To cover the traumatic wound