Frequent Tail-tip Blood Sampling in Mice for the Assessment of Pulsatile Luteinizing Hormone Secretion

Summary

Here we present a tail-tip blood sampling protocol for frequent sample collection in unrestrained mice. This method is useful for assessing patterns of pulsatile luteinizing hormone secretion and could be adapted for analysis of other circulating factors.

Abstract

In many endocrine systems, circulating factors or hormones are not released continuously, but are secreted as a discrete pulse in response to a releasing factor. Single-point sampling measures are inadequate to fully understand the biological significance of the secretory pattern of pulsatile hormones either under normal physiologic conditions or during conditions of dysregulation. Luteinizing hormone (LH) is synthesized by the anterior pituitary gonadotrope cells and secreted in a pulsatile pattern which requires frequent collection of blood samples for pulse assessment. This has not been possible in mice until recently, due to the development of a high-sensitivity LH assay and advancement in a technique for frequent low-volume sample collection, initially described by Steyn and colleagues.¹ Here we describe a protocol for the frequent peripheral blood sample collection from mice with sufficient handling acclimatization to detect pulsatile secretion of LH. The current protocol details an expanded acclimatization period that allows assessment of robust and continuous pulses of LH over multiple hours. In this protocol, the tip of the tail is clipped and blood is collected from the tail using a hand-held pipette. For assessment of pulsatile LH in gonadectomized mice, serial samples are collected every 5-6 min for 90-180 min. Importantly, the collection of blood and measurement of robust pulses of LH can be accomplished in awake, freely behaving mice, given adequate handling acclimatization and effort to minimize environmental stressors. Sufficient acclimatization can be achieved within 4-5 weeks prior to blood collection. This protocol highlights advances in the methodology to ensure collection of whole blood samples for assessment of pulsatile LH secretion patterns over multiple hours in the mouse, a powerful animal model for neuroendocrine research.

Introduction

Gonad function in mammals is dependent upon gonadotropin secretion, luteinizing hormone (LH) and follicle stimulating hormone, from the pituitary gland. The gonadotropins are secreted in either a pulsatile or surge pattern in response to hypothalamic secretion of gonadotropin-releasing hormone (GnRH). The synthesis and secretion of both LH and FSH are regulated via endocrine, paracrine and autocrine action from a variety of molecules including hypothalamic GnRH, gonadal steroid hormones, and the activin-inhibin-follistatin system, as well as a myriad of physiological conditions including stress and energy balance.²

The pulsatile pattern of LH in blood arises from a rather abrupt discharge of LH into peripheral blood, followed by approximately exponential elimination. Important features of the pattern include the frequency of each LH discharge and the amplitude of the LH response, both of which are dictated, in part, by the release of GnRH. Due to the difficulty in collecting hypothalamic-pituitary portal blood for measurement of pulsatile GnRH, the sampling and measurement of LH is used as a proxy for GnRH regulation of the hypothalamic-pituitary-gonadal axis. Therefore, critical information is encoded in the frequency and amplitude of LH pulses, which cannot be determined from a single sample.

Analysis of pulsatile LH secretion has historically been limited to large mammals (humans, primates, and sheep) due to their large blood volume and tolerance for frequent blood sample collection. In rodents, frequent blood sampling was limited to the rat and achieved via indwelling atrial catheter.^3,4 The relatively low cost and availability of genetic (e.g. cre-lox, CRISPR) and complex neural circuit (e.g. optogenetics, chemogenetics) manipulations make mice an attractive model organism; however, attainment of frequent blood samples and subsequent analysis of LH concentrations has until recently, proven elusive. This monumental task was pioneered by Steyn and co-workers.¹ Since then, several labs have begun to utilize frequent blood sampling and ultra-sensitive LH assays to assess pulsatile LH secretion in a variety of experimental paradigms.^5,6,7,8,9 It should be noted that the pursuit of a practical method of collecting multiple blood samples from mice has been in progress for at least 40 years¹⁰ with multiple refinements made along the way.^11,12

Assessment of LH pulse patterns (i.e. frequency and amplitude) represents a major refinement in monitoring basal gonadotropin secretion in this genetically tractable animal model. Traditionally, LH concentrations in mice were determined in a single blood sample. One weakness of single-point samples is a highly variable data set because LH concentrations are naturally fluctuating during each pulse. Another weakness is that isolated measurements inherently miss critical information conveyed by the patterns of LH pulse secretion. Thus, a method for collecting frequent blood samples in freely behaving, unrestrained mice (except for gentle handling during sampling) will provide enhanced information and prove useful to many laboratories investigating pulsatile hormone regulation.

Here, we describe a protocol for the collection of frequent (every 6 min) blood samples from awake, unrestrained mice. Importantly, we include a handling acclimatization protocol that allows for robust and continuous detection of pulsatile LH secretion in whole blood samples collected over a length of time in which pre- and post-assessment to an acute challenge can be determined, such as the response to the psychosocial stress of immobilization and restraint. An effective assay for LH concentrations from whole blood samples has been described previously;¹ this protocol is focused on a method for collecting the blood samples for LH pulse measurement.

Protocol

The method described here is in agreement with the National Institutes of Health Animal Care and Use Guidelines and have been authorized by the Institutional Animal Care and Use Committee at the University of California, San Diego.

1. Acclimatization to Handling

1. Handling procedure
   1. Place mouse cages in the biosafety cabinet. Remove the first mouse from the cage and place on a suitable surface (e.g. a clean cage lid) within the biosafety cabinet.
   2. Gently restrain the mouse on the work surface by holding the base of the tail with the forefinger and thumb of one hand. Then, firmly stroke the ventral surface of the tail, from the base to the tip of the tail, with the forefinger and thumb of the other hand. Repeat this stroking 6 times (i.e. 1 set) and return the mouse to its cage.
   3. Wait 6 min and repeat step 1.1.2.
      NOTE: In total, step 1.1.2 will be repeated 4 times per mouse (i.e. 4 sets of 6 strokes), so that each mouse will receive a total of 24 tail strokes on each day of handling.
2. The frequency of daily handling
   1. From five until two weeks before the planned blood collection day, handle mice as described in step 1.1, five days per week (mice are not handled on Saturday or Sunday until the final two weeks of acclimatization).
   2. If experimental treatment during the sampling period will include any additional handling (e.g. scruffing or intraperitoneal injection), acclimatize the mice to this handling activity during each handling session.
      Note: For acclimatization to injection procedures, use a blunted needle to perform a sham injection.
   3. During the two weeks before the planned blood collection day, handle mice as described in 1.1, seven days per week.
   4. At least two weeks before the planned blood collection day, house mice in pairs to minimize disruptions to the mice during sampling.

2. Preparation of Blood Collection Tubes

1. Prepare ultrasensitive LH assay buffer in a glass bottle: 0.2% bovine serum albumin and 0.05% Tween-20 in PBS [0.2 g KCl, 8 g NaCl, 1.44 g Na₂HPO₄ (anhydrous), 0.24 g KH₂PO₄, ultrapure water to 1 L, pH 7.4, filter and autoclave], store at 4°C.¹
   NOTE: Volume of ultrasensitive LH assay buffer to be prepared can be calculated based on the number of samples and the volume per sample as indicated below (2.2 & discussion)
2. Prepare blood collection tubes (0.6mL microcentrifuge tubes). Label tubes and aliquot assay buffer (57 µL of buffer per tube; note, this volume may vary depending on the volume of blood collected or the ratio of the blood to the buffer desired). Tubes can be prepared days ahead of sampling, store at 4°C.

3. Blood Collection

1. Preparation of blood collection materials.
   1. Prepare biosafety cabinet for use, and arrange the following materials in the hood or on a cart nearby: 10 µL pipette (set to 3 µL or desired blood collection volume), pipette tips, waste bin for used pipette tips, timer, printout with animal numbers and sample numbers (for notes regarding sampling or animal issues), ice bucket with blood collection tubes, scissors, and small gauze (2" x 2").
      NOTE: The "count up" function on a laboratory timer is useful because it does not have an audible alarm that could disturb the mice
   2. Use a permanent marker to mark the tail of each mouse (near the base) to assist with rapid identification of the correct mouse during sampling.
2. Clipping of the tail and pre-blood collection preparation.
   1. At 45 min before the start of the blood collection, remove the first mouse from its cage and place on a suitable surface (a clean cage lid works well) within the biosafety cabinet.
   2. Use sharp, sterile scissors to remove 1-2 mm of the tip of the mouse tail, following aseptic preparation (i.e. scrub with alcohol and betadine).
      NOTE: This can be accomplished in awake animals with gentle restraint or under isoflurane anesthesia.  Additionally, analgesia may be provided following the recommendation of the local IACUC.
   3. Carefully stroke the tail of the mouse as described above (1.1.2; 1-2 strokes are generally sufficient) until the droplet of blood forms on the tail tip.
   4. Use a pipette with a clean tip to collect 3 µL of blood from the tail tip and discard the pipette tip with blood.
   5. Before returning the mouse to its cage, ensure that blood flow has stopped. If necessary, apply gentle pressure with sterile gauze.
   6. Repeat steps 3.2.1 - 3.2.5 for all mice. Subsequent blood samples can be collected by firmly stroking the mouse's tail until a droplet of blood forms at the tip of the tail.
      NOTE: If a blood droplet does not form after firm strokes, the tail can be dabbed with a gauze pad soaked in saline. Clots are more likely to form during less frequent sampling (i.e. >15 min intervals). Once the clot is cleared from the vein, sampling can continue.
   7. Continue to collect 3 µL of blood from each mouse as described above every 6 min for approximately 45 min during this pre-blood collection preparation period. Discard the blood and pipette tip.
3. Blood sampling
   1. Collect 3 µL of blood from the tail tip as described above. Take caution to ensure that the entire 3 µL sample is taken into the pipette tip (without bubbles or bedding contamination). Eject the blood sample into the assay buffer in a labeled tube. Mix by inversion and return the tube to ice.
   2. Before returning the mouse to its cage, ensure that the blood flow has stopped. If necessary, apply gentle pressure with sterile gauze.
   3. Repeat steps 3.3.1 - 3.3.2 for each mouse, every 6 min, for the predetermined sampling duration. Monitor each animal for signs of distress (e.g. partially closed eyelids, hunched position [not caused by other treatment] or lack of response to handling) and terminate sampling, if necessary.
      NOTE: Behavioral distress or other complications that require termination of sampling occur extremely rarely in our laboratory.
   4. If animals are not euthanized following blood sampling, ensure that the blood flow from the tail-tip has completely stopped. Wipe any spilled blood from the inside of each animal's cage (or change cages) and return the animal cages to the housing rack.

4. Sample Processing and Analysis

1. Store blood samples at -20 °C until analysis.
   NOTE: LH is assayed in whole blood samples diluted in assay buffer; no separation of sera or plasma is required prior to storage or analysis.
2. Assay blood samples by ultrasensitive ELISA as described previously¹ and report values in ng/mL of whole blood following correction for dilution of the sample volume in the assay buffer.
3. Identify LH pulses in the data set. Calculate and compare mean pulse amplitude and pulse frequency (or inter-pulse interval) as appropriate for the data set.
   NOTE: Published criteria^13,14 and programs,^15,16 for detecting LH pulses are available.

Results

Representative LH pulse patterns from 4 mice are shown in Figure 1 (data reprinted from Yang et al., 2017). LH was measured in frequent blood samples to determine the response to an acute psychosocial stress challenge. Adult female C57/Bl6 mice were ovariectomized and handled as detailed in this protocol for frequent blood collection. Blood samples were collected for the first 90 min in all animals to establish a pre-treatment baseline of LH pulsatil...

Discussion

Here we describe a protocol for frequent blood collection of whole blood tail-tip samples for assessment of pulsatile LH secretion in mice. This protocol enables the collection of samples for detection of acute changes in pulsatile LH secretion following exposure to psychosocial stress and is well-suited for assessment of LH pulses under other acute or chronic manipulations.

A critical component of this protocol for achieving reliable and robust profiles of LH pulses is the handling acclimatiz...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Biosaftey cabinet	Lab Products Inc	L/F-B
Bovine serum albumin	Sigma	A5403
Tween-20	Sigma	P2287
KCl	Sigma	P9333
NaCl	Sigma	S7653
Na2HPO4 (anhydrous)	Sigma	S7907
KH2PO4	Sigma	P5655
Ultrapure water	Millipore		Purified and filtered water
Broome Rodent Restraint Device	Harvard Apparatus	52-0460	Not necessary for blood collection, but were used in the collection of representative data.
DynPeak	n/a	n/a	http://journals.plos.org/plosone/article?id=10.1371/journal.pone.0039001