Blood Collection (Guideline)

Guidelines:The IACUC has provided a set of guidance documents (Policies, Guidelines, and Informational Sheets) for use when planning animal procedures at the University of Iowa. An exception to a Guideline must be described and justified in the Animal Protocol and approved during the normal review process.

 

Purpose:

This document provides direction and guidance on appropriate blood collection methods and volumes for animals used in research at the University of Iowa. These guidelines are intended for use by qualified personnel performing blood collection as described on an IACUC-approved Animal Protocol.

There are several factors to consider when determining the appropriate blood collection volume and technique. These include:

• The species to be sampled
• The size of the animal to be sampled
• The age and health of the animal to be sampled
• The minimum volume required for analysis
• The frequency of sampling necessary
• The training and experience of the personnel performing the collection
• The suitability of sedation and/or anesthesia

The sample volume selected should always be the minimum volume of blood which satisfies experimental needs. Appropriate restraint (physical or chemical) should be employed to minimize risk of injury to the animal and personnel.

Guidelines for calculation of collection volume:

• The maximum permitted blood volume includes blood lost during collection.
• As a general rule, 20 drops = 1 mL (i.e. 5 drops = 250 uL)

Maximal blood collection limits are as follows:

• No more than 1% of the animal’s body weight in one collection or over a 24 hour period
  • For example: 25g mouse x 1% = 0.25mL or 250uL maximum blood removal
• No more than 1.5% of the animal’s body weight in two weeks (14 days)
  • For example: 200g rat x 1.5% = 3.0mL maximum over 14 days

Frequent Rodent Calculations

Mouse

Weight	Maximum blood loss at one time/ in 24 hours	Maximum blood loss  over 14 days
20 g	200 uL	300 uL
25 g	250 uL	375 uL
30 g	300 uL	450 uL

 

Rat

Weight	Maximum blood loss at one time/ in 24 hours	Maximum blood loss  over 14 days
200 g	2.0 mL	3 mL
250 g	2.5 mL	3.75 mL
300 g	3.0 mL	4.5 mL

 

Common Blood Collection Routes By Species

Mouse

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Submandibular vein
Tail vein* (see below)
Saphenous vein
Retro-orbital sinus (see below)		Yes
Cardiac (non-survival)		Yes

 

Rat

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Tail vein
Saphenous vein
Jugular vein	Yes
Retro-orbital plexus (see below)		Yes
Sublingual vein	Yes
Cardiac (non-survival)		Yes

 

Ferret

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Cephalic vein
Saphenous vein
Jugular vein	Yes
Cranial vena cava	Yes

 

Rabbit

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Marginal ear vein
Central auricular artery
Saphenous vein	Yes
Jugular vein	Yes
Cardiac (non-survival)		Yes

 

Hamsters

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Saphenous vein
Cephalic vein
Jugular vein	Yes
Cranial vena cava	Yes
Cardiac (non-survival)		Yes

 

Guinea Pigs

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Ear vein (droplet)
Saphenous vein
Cranial vena cava	Yes
Cardiac (non-survival)		Yes

 

Gerbils

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Lateral saphenous vein
Cranial vena cava	Yes
Cardiac (non-survival)		Yes

 

Xenopus

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Dorsal tarsal vein		Yes
Cardiac (survival)		Yes
Cardiac (non-survival) (also tadpoles)		Yes

 

Pigeon

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Brachial wing vein	Yes

 

Dog or Cat

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Cephalic vein
Saphenous vein
Jugular vein
Cardiac (non-survival)		Yes

 

Pigs

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Ear vein	Yes
Cranial vena cava	Yes
Jugular vein	Yes
Cardiac (non-survival)		Yes

 

Ruminants

Common Blood Collection Route(s)	Sedation Recommended	Anesthesia Required
Jugular vein
Lateral saphenous vein
Tail vein
Ear vein

 

Restraint and anesthesia for blood draws:

Restraint methods and anesthesia used to collect blood on research animals must be described and approved in the animal protocol. Examples of restraint devices include rodent restraint tubes, surgical towel or decapicones.

 

Hemostasis:

Assuring that blood flow has stopped (hemostasis) is of upmost importance after collecting a blood sample. To achieve hemostasis, place gentle pressure over the site of blood collection to stop the bleeding. A gloved hand and a piece of gauze are commonly used. Best practice involves re-inspecting animals approximately 5 minutes after return to their cage to assure blood flow has stopped. 

Tail vein collection definitions:

Tail vein collection is defined as use of a hypodermic needle or lancet to access the tail vein along the body of the tail. 

Tail transection (also referred to as tail snip or clip) is NOT considered a routine method of blood collection and should be described as a non-surgical procedure with associated monitoring and pain management where appropriate.

• Blood collection of animals greater than 24 days of age
  • Use of a systemic analgesic given prior to tail snipping is required.
    • systemic analgesic examples: carprofen, meloxicam, buprenorphine, etc
    • Analgesics such as lidocaine or bupivacaine are considered local analgesics and when administered alone, do not provide optimal pain management for this procedure.
  • Tail snipping for blood collection at this age is potentially painful and should be avoided if possible.
• More than one sample over the life of the animal:
  • Limit of two collections, no more than a total of 2-5mm of the distal tail removed over all collections (including tail snipping for genotyping purposes)
  • Use of a systemic analgesic given prior to tail snipping is required.

Techniques for tail vein dilation:

The following techniques may be used to increase blood flow on the tail vein of a mouse or a rat:

1) Use of a heating lamp*

2) Submerging the tail in warm water (no warmer than 40^oC/104^oF) *

3) Placing rubbing alcohol over the tail

* Animals under a heat lamp must be under direct supervision and care must be exercised to prevent overheating an animal. Animals that overheat may show an increased respiratory rate, decreased movement, red extremities and avoidance of the heat lamp. 

Retro-Orbital Sampling:

Retro-orbital blood collection in rodents can provide moderate to large amounts of blood when performed by well-trained personnel. However, severe injuries may occur to the animal if this procedure is not done properly, and available alternatives should be used whenever possible.

The use of retro-orbital bleeding must be described in the protocol and approved by the IACUC. Because rats have a venous plexus rather than a sinus (as in the mouse), the use of this method may result in greater tissue damage and alternative collection sites are strongly recommended.

If retro-orbital collection is necessary, the following guidelines apply:

• General anesthesia is required
• Microhematocrit tubes that hold 50-75 microliters are recommended to minimize risk of injury
• Only one eye may be sampled at any time
  • If attempted collection from one eye is unsuccessful, an alternate method approved in the Animal Protocol (e.g. submandibular or saphenous route) must be used, rather than reattempting retro-orbital collection from the same or opposite eye

• Alternate between left and right eyes per session

• No more than 1 collection performed per 7 days (alternate eyes). therefore 14 days between collections in the same eye
  • Exception: If repeated sampling within 8 hours is necessary and approved in the Animal Protocol, the retro-orbital sinus may be re-sampled by disrupting the blood clot (from the original collection site) without repeated damage to the sinus, provided the 24 hour maximum blood collection limits are not exceeded
    • Please consult with veterinary staff for demonstration and training of proper technique to reduce risk of trauma

• A maximum of 3 procedures may be performed per eye (up to 6 collections total)

• If injury and/or rupture of the eye or surrounding tissues occurs due to this method, the animal must be immediately euthanized or an OAR veterinarian consulted for guidance

Application of a topical ophthalmic anesthetic during/after collection should be considered to provide post-procedural analgesia.
 

Last Reviewed by the IACUC 07/17/2023