Microscopic Observation of Lymphocyte Dynamics in Rat Peyer's Patches

Summary

Here, we describe a precise method for collecting thoracic duct lymphocytes and observing the migration of gut-tropic lymphocytes in rat Peyer’s patches for 3 hours using time-lapse photography. This technique can clarify how the dynamics of lymphocytes are affected under inflammatory conditions.

Abstract

Naïve lymphocytes recirculate from the blood to the lymphoid tissues under physiological condition and it is commonly recognized as an important phenomenon in the gut immunity. The stroma of secondary lymphoid organs, such as Peyer’s patches (PPs) or mesenteric lymph nodes, are where naïve lymphocytes sense antigens. Naïve lymphocytes circulate through the bloodstream to reach high endothelial venules, the portal of entry into PPs. Some immunomodulators are estimated to influence lymphocyte migration, but the precise evaluation of microcirculation dynamics is very difficult, and establishing a method to observe lymphocyte migration in vivo can contribute to the clarification of the precise mechanisms. We refined the method of collecting lymphocytes from the lymph duct and observing the detailed dynamics of gut-tropic lymphocytes in rat PPs. We chose confocal laser scanning microscopy to observe rat PPs in vivo and recorded it using time-lapse photography. We can now obtain clear images that can contribute to the analysis of lymphocyte dynamics.

Introduction

Peyer’s patches (PPs) consist of hundreds of lymphoid follicles in the lamina propria of the small intestine. PPs are divided into follicles, the interfollicular region, and germinal centers located in the lower part of the follicles, where lymphocytes are stimulated by antigen presentation. There are no afferent lymphatic vessels, and the antigens invade the lamina propria from the intestinal lumen via the epithelial cell layer. The epithelial region covering lymphoid follicles is called the follicle-associated epithelium, within which specialized interspersed M cells uptake mucosal antigens. M cells take in antigens from the luminal side and antigens are then captured by dendritic cells and presented toward naïve lymphocytes that flow into PPs through the endothelium of high endothelial venules (HEVs)¹. PPs play an important role in intestinal immunity and are related with the early stage of inflammation. Many molecular interactions involve the entrance of lymphocytes to secondary lymphoid organs (SLOs), including adhesion molecules, chemokines^2,3, and sphingosine-1-phosphate⁴; thus, there are many expected therapeutic targets. Therefore, observing the lymphocyte dynamics within PPs enables us to catch a glimpse of the very early stage of inflammation and examine the usefulness of several promising drugs.

The method here focuses on the migration of lymphocytes in PPs, which includes several procedures (cannulation into the thoracic duct⁵ and collecting lymphocytes and long-term observation after the injection into collected lymphocytes). Since these procedures are complex and it was difficult to see exactly how each procedure was performed in previous reports, we mentioned here some tips to achieve a successful observation. For example, cannulation of the tubes into the thoracic duct was very difficult, and the initial success rate of cannulation was less than 50%. However, we improved the method and achieved a success rate exceeding 80%. We mentioned some other tips in this manuscript that are necessary for the successful observation to enable the quantitative evaluation of the transendothelial migration of lymphocytes under several conditions.

In previous reports, it was difficult to understand the three-dimensional changes over time, such as the intravenous injection of India ink to stain the vascular structure of PPs⁶, or the microscope being monofocal⁷. In recent years, an observational method using some photoconvertible fluorescence protein transgenic animals such as Kaede mice have clarified systematic cellular movements in vivo⁸. The other study clarified CD69 independent shutdown of lymphocyte egress from PPs⁹. We used confocal laser scanning microscopy (CLSM) because of its high analytical capability. Now we can easily obtain high-resolution images and use them to analyze lymphocyte dynamics.

In this report, we demonstrated a series of methods for evaluating lymphocyte migration in PPs. First, we showed refined methods of thoracic duct cannulation to collect lymphocytes. Second, we improved the observational methods in several ways to maintain objective organs whenever possible under microscopic observation, enabling us to obtain high-quality images for 3 hours. Third, we quantified the cellular movements of lymphocyte migration to evaluate the effects of some medications. These modified protocols will contribute to development of mucosal immunology evaluations.

Protocol

The experimental protocol was approved by the Animal Research Committee of National Defense Medical College (no. 16058). The animals were maintained on standard laboratory chow (CLEA Japan Inc, Tokyo, Japan). The laboratory animals were treated in accordance with National Institutes of Health guidelines.

1. Collection and separation of lymphocytes

NOTE: Since lymphocytes must be fresh and cannot be stored, they must be collected from rats for each experiment. In addition, gut-tropic lymphocytes must be collected directly from the thoracic duct where they circulate. All procedures are expected to be completed within 6 hours, and all instruments, gloves, and surfaces are clean. In order to keep the animals in a physiologically stable state, all saline and other fluids used in the experiment should be kept warm.

1. Form a cannulation tube (1 mm diameter) like a heparin curve (a radius of about 5 mm) after dipping it in hot water (about 80–90 °C) and fix it to a plastic board using adhesive tape for a few hours in advance.
2. Anesthetize a male Wistar rat (8–12 weeks) with intraperitoneal injection of a mixture of Midazolam (2mg/kg), Domitor (0.15mg/kg), and Betulphar (2.5mg/kg) and cut the body hair of the abdomen using a hair clipper. Remove the hair firmly after shaving so that the hair does not enter the abdominal cavity.
3. After confirming that the stable depth of anesthesia required for the procedure is obtained by toe pinch, make an incision with surgical scissors horizontally from midline to the left subcostal area. Be careful not to damage the blood vessels in the parietal peritoneum by watching the vessels under light.
4. Wrap the stomach with wet gauze and move the stomach gently to the right outside of the body to reveal the retroperitoneal organs. Insert a notch between the erector muscles of the spine and the adipose tissue using surgical scissors and bluntly separate them with fingers.
5. Carefully strip off the connective tissue around the thoracic duct. The excess connective tissue increases with age. Expose the thoracic duct from just beneath the left crus of the diaphragm caudally until a 20 mm length of the thoracic duct was visible. Gently separate adhesions between the thoracic duct and aorta using precision tweezers or wet cotton swabs.
   1. Perform this process carefully because some rats have arterioles branching from the abdominal artery crossing over the thoracic duct or a short thoracic duct due to a higher position of the lymph plexus (small thoracic ducts spreading like spider webs). Avoid unnecessary contact to the thoracic duct to avoid inducing edema.
6. Apply a ligature by a string (3-0 silk) on the thoracic duct just beneath the left crus of the diaphragm. The caudal thoracic duct becomes distended.
7. Make a hole (5 mm diameter) in the abdominal wall by stabbing the cutting edge of surgical scissors, pass the hairpin-curved cannulation tube, and ligate the tube on the iliopsoas muscle at one point. Fill the cannulation tube with normal saline containing 10 U/mL heparin.
8. After placing a string (3-0 silk) beneath the distended thoracic duct, stab the thoracic duct with the sharply cut edge of a cannulation tube, cannulate it toward the tail about 5 mm, and ligate the thoracic duct with cannulation tube for fixation.
9. To supply saline to prevent dehydration, create a hole (3 mm diameter) on the anterior wall of the antrum of the stomach using precision tweezers and pass the silicon tube (2 mm in diameter) to the duodenum through the pyloric ring. After stitching up a wound and maintaining the animals in Bollman’s cages, start to infuse sugar-laden saline into each rat’s duodenum from the silicon tube at a flow rate of 3 mL/h. Cover the entire cage with a paper towel to keep it warm.
10. Fix the cannulation tube to the hole in the center of the lid of a 50-mL conical tube on ice containing 6 U/mL heparin, 10% fetal bovine serum, and RPMI 1640 medium (pH 7.4; see the table of materials), and collect thoracic duct lymphocytes (TDLs) on ice. Be careful not to contact the tip of the tube to the wall of the conical tube to prevent cannulated-tube occlusion due to fibrin clot formation inside the tube. Lymph fluid (about 20 mL) including about 1.0 x 10⁸～10⁹ lymphocytes can be obtained in 6 hours. To obtain the lymphocytes  under complete anesthesia, plane of anesthesia is monitored and lymph flow is observed appropriately. The same anesthetics are added at the same dose about 3 hours after rats are put into Ballman's cage to obtain deep anesthesia continuously for 6 hours.

2. Lymphocyte labeling with carboxyfluorescein diacetate succinimidyl ester (CFDSE)

1. Dissolve CFDSE (Table of Materials) in dimethyl sulfoxide (DMSO) to 15.6 mM (500 µg of CFDSE dissolved in 60 µL of DMSO).
2. Incubate lymphocytes (1 x 10⁸～10⁹) in 50 mL of RPMI 1640 with 50 µL of CFDSE solution for 30 min at 37 °C as described previously¹⁰.

3. Experimental setup for microvascular studies

1. Anesthetize recipient rats (8–12 weeks) with intraperitoneal injection of a mixture of Midazolam (2mg/kg), Domitor (0.15mg/kg), and Betulphar (2.5mg/kg) and confirm the depth of anesthesia by toe pinch. Wet the abdomen before grooming the fur to minimize hair contamination. Then open the abdomen of the recipient Wister rat via a midline incision.
2. Put a rat on a portable stainless-steel plate (about 120 x 300 mm) with a rectangle hole around the center covered with a glass slide (24 x 50 mm). Choose about 10 cm of the ileal segment including PPs for observation.
3. Keep the intestine as warm as possible and moist with phosphate buffered saline (PBS) warmed to 37 °C. Soak gauze that is used to cover the small intestine with PBS.
4.  While giving continuous anesthesia with 2 % isoflurane (see table of materials), put the slide on the stage of the microscope and choose suitable areas for observation of the microcirculation in PPs where some HEVs are running through the serosa. PPs range in size; larger ones are suitable for observation of the microcirculation using CLSM. The small intestine is not straight in places; a straight segment at least 2 cm long without any tension is suitable for observation.
5. Cover the adjacent intestinal segment and mesentery with absorbent cotton soaked with PBS. Place the intestine segment between two rolled cotton balls and position it as far as possible from the rat’s body to prevent it from being vibrated by the rat’s heartbeat and breathing.
6. Using a 1 mL syringe, slowly inject (over 1 min) CFSE-labeled TDLs (1 x 10⁸ cells) into the jugular vein of the recipient rats. A rapid intravenous injection may influence the systemic circulation.

4. Microcirculation of lymphocytes

1. Continuously monitor TDLs in the microvasculature of PPs using CLSM and record on a computer for 3 hours using time-lapse photography at 30 s intervals. The depth from the serosa to the HEV of PPs is about 25 μm, enabling the observation of the stroma and capillary lymph vessels to a depth of 30 μm.
2. Inject Texas Red–dextran (25 mg/kg) into the jugular vein of each recipient rat to stain the bloodstream and Hoechest 33342 (5 mg/kg) to stain the cell nuclei.
3. (Optional) To quantify lymphocyte dynamics, define lymphocytes adhering to HEVs more than 30 seconds as “adhesive lymphocytes” and lymphocytes emigrating from HEVs to stroma as ‘‘migrating lymphocytes”. Then calculate the average percentage of migration (migrating lymphocytes / adhesive lymphocytes + migrating lymphocytes) per field of vision (approximately 0.3 mm²).

Results

Collecting lymphocytes from lymph
To prepare the rat for thoracic duct cannulation, make an incision in the tense thoracic duct as shown in Figure 1 and then maintain the rat in a Bollman’s cage as shown in Figure 2.

When the lymphocytes are well collected, we can obtain about 20 mL/6 h lymph fluid containing about 10⁷～10⁸/mL lymphocytes. Of the TDLs, 70% express CD4, among whi...

Discussion

Here we described a protocol for collecting naïve gut-tropic lymphocytes and observing their migration in rat PPs. These procedures can reveal how lymphocytes move in the microvasculature of PPs and make it possible to visually compare their dynamics under a normal or medicated condition. The direct observation of these dynamics has much merit to obtain a clue for immunological modification by some drugs, although the observational period is limited to only a few hours.

We mentioned some ...

Materials

Name	Company	Catalog Number	Comments
A1R+	Nikon		Comfocal Laser Scanning Microscopy
Carboxyfluorescein diacetate succinimidyl ester	Thermo Fisher Scientific	C1157
Hoechest 33342	Thermo Fisher Scientific	H3570
Isoflurane	Wako Pure Chemical Industries	099-06571
RPMI 1640 medium	GIBCO	11875093
Texas Red–dextran	Thermo Fisher Scientific	D1863