mouse microsurgery and echocardigraphy
DESCRIPTION
Our mouse microsurgery and echocardiography workshop is designed for researchers to learn surgical techniques commonly used in cardiovascular and cerebrovascular research. Participants will learn survival and non-survival surgeries; also they will learn intravenous drug injection, blood collection, jugular vein catheterization (acute and chronic). They will learn intubation, anesthesia, surgical monitoring (including body temperature, EKG, heart rate) techniques which are commonly used during survival surgeries. All participants will have a chance to use real working pressure and pressure-volume catheters for measuring blood flow, blood pressure and left ventricular pressure-volume loops. Using transthoracic echocardiography, participants will learn cardiac systolic and diastolic function measurement. Using pulsed wave Doppler echocardiography, participants will learn blood flow velocity measurement. Echo-guided pressure/volume catheter insertion into left ventricle will allow participants to record left ventricular pressure, pressure-volume loop, also record pressure-volume loop changes during stress echocardiography. By using contrast echocardiography they will learn myocardial blood flow measurement. Participants will also learn how to identify tumor size and tumor blood flow measurement by using contrast echocardiography These are a hands-on sessions and participants will practice on mice. After survival surgery they will learn postsurgical care. The last day of the workshop, we will measure cardiac function after survival surgeries (myocardial infarction and transaortic banding) using echocardiography. For this workshop we are going to use Visual Sonic Vevo 2100, VEVO-770 and Siemens Acuson Sequoia 512 ultrasound systems.TRANSCRIPT
Day 1
Northeast Ohio Medical University
Rootstown, Ohio, 44272
MouseMicrosurgery workshop
We would like to thank the following companies for supporting and sponsoring this workshop
Survival surgeries
• Myocardial infarction
• Transaortic banding and de-banding
If mouse survives after the surgery, we will keep the mouse until last day of the workshop. We will do echocardiography all mice survived after surgery. Echocardiography will approve the size of the infarction and the degree of transaortic constriction.
Day 1• Day One
• 8-8:30 a.m.
• Introductions
• 8:30-9:30 a.m.
• Acute and Chronic Surgery
• Anesthetics and Analgesics
• Post-surgical care and monitoring
•
9:30-10 a.m.
• Coffee break
• 10 a.m. - Noon
• Demonstration of the following:
• Dissection of vessels in mice(femoral artery and cartoid artery)
• Mouse jugular vein catheterization
• Pressure measurement (from femoral or cartoid arteries)
• Pressure volume measurement
• Noon - 1:30 p.m.
• Lunch
• 1:30- 5 p.m.
• Practical session: Participants will select the type of vessel he or she would like to practice
• Demonstration: Femoral artery blood flow and pressure measurement; computerized data collection. Participants who are interestedcan follow this demonstration.
• 5 - 5:30 p.m.
• Questions and Answer Session
Day 1Surgical Instruments:• List of necessary instruments for mouse surgery• Care and cleaning, sterilization
Surgical Station:• Table (heated and non-heated)• Securing animals on the surgical table• Hair removal and preparation of surgical region
Microscopes:• Type of microscopes needed for the surgery• Lighting sources• Depth of field, field of vision
Acute and Chronic Surgery:• Aseptic technique, sterilization methods• Sutures and suturing techniques• Catheter material and manufacture
Anesthetics and Analgesics:• Types of anesthetic for surgery• Types of analgesics for chronic surgery• Postoperative care (chronic procedures)• Respirators and ventilators for anesthesia
Surgical tools
Care and cleaning
• Before the surgery, check the list of surgical tools you need.
• Quality is important , not quantity. Quality of surgery highly depends on quality of instruments. It saves times, animals, and money.
• During the surgery keep only the surgical tools you need. Excess of surgical tools will make your table messy and it will be hard to find the tool you need.
• Take care of your instruments. Micro-scissors dull easily. This will compromise cutting blood vessels for cannulation. Micro-forceps bend easily, and a bent forceps will not hold tissue.
• After every surgery wash and dry your instruments. Take special care during washing, otherwise it is easy to break and/or bend micro-forceps and micro-scissors.
• Use Alconox or Alcotabs. Immerse the instrument for 5-10 minutes in this solution. This will help to remove the blood from the tools.
• Use soft brush (tooth brush is good) or surgical gauze for washing.
• Keep locks and ratchets open during cleaning. After cleaning rinse your tools in deionized/distilled water.
• Store the instruments in a sterilization box, and then put them into the drying oven or autoclave using the drying cycle.
• It is best to store micro-instruments in a locked drawer as they have a tendency to develop “legs.”
Care and cleaning
Loaning your instruments to “Friends”- NEVER!!! And the answer is: -I would, if I could, but unfortunately I cannot. But if you have extra tools, always help your friends!
Care and cleaning
N E V E R !!!Curved forceps
25-$80 or more
Dumont #5 Forceps
$25-$60 or more
Spring Scissors
$270-$420 or more
A B C
D E F
Care and cleaning
Cover the tips of micro-scissors and micro-forceps with plastic or rubber caps
N E V E R !!!
AB
C D
Day 1Surgical Instruments:• List of necessary instruments for mouse surgery• Care and cleaning, sterilization
Surgical Station:• Table (heated and non-heated)• Securing animals on the surgical table• Hair removal and preparation of surgical region
Microscopes:• Type of microscopes needed for the surgery• Lighting sources• Depth of field, field of vision
Acute and Chronic Surgery:• Aseptic technique, sterilization methods• Sutures and suturing techniques• Catheter material and manufacture
Anesthetics and Analgesics:• Types of anesthetic for surgery• Types of analgesics for chronic surgery• Postoperative care (chronic procedures)• Respirators and ventilators for anesthesia
Surgical Station:
• Table (heated and non-heated)- During the surgery it is very important to monitor animals body temperature. Because of the small size, mice are losing body temperature very fast. It is very important to keep the animals in warm area after the surgery, during the recovery period. Be very carefully from overheating the animals.
• Securing animals on the surgical table - Non-obese animals you can secure on surgical table using taps(Figure 1) . Hair removal and preparation of surgical region- For hair removal ChroMini Cordless Clipper (Harvard Apparatus #341414, Figure 2A).
Chemical hair removal (Nair, from any store) can also be used. Clean the skin well after using NAIR(Figure 2B). If the NAIR stays on skin, it can cause irritation and inflammation of skin.
For survival surgery, clean the skin with 1) 70% ethanol, 2) with betadine, and 3)with 70 % ethanol again . After preparing the skin, cover the mouse with surgical towel(Figure 3).
Figure 1 Figure 2 Figure 3
A B
Day 1Surgical Instruments:• List of necessary instruments for mouse surgery• Care and cleaning, sterilization
Surgical Station:• Table (heated and non-heated)• Securing animals on the surgical table• Hair removal and preparation of surgical region
Microscopes:• Type of microscopes needed for the surgery• Lighting sources• Depth of field, field of vision
Acute and Chronic Surgery:• Aseptic technique, sterilization methods• Sutures and suturing techniques• Catheter material and manufacture•
Anesthetics and Analgesics:• Types of anesthetic for surgery• Types of analgesics for chronic surgery• Postoperative care (chronic procedures)• Respirators and ventilators for anesthesia
Microscopes:
• Type of microscopes needed for the surgery
Leica/Nikon/Zeiss/ Olympus/AmScope and many other companies have dissecting and surgical
binocular and trinocular microscopes. During microscope selection always pay attention on
working distance (more than 30 mm)
• Lighting sources(Figure 3)
• Depth of field- When working, select the largest possible working distance which will still permit
you to assume a comfortable working position. This offers the benefit of a good depth of field
and sufficient space for instrumentation
• Field of vision- is the area that is visible to you when you look through the microscope
eyepieces. When you increase the magnification, you are focusing in on a smaller area.
Figure 1 Figure 2
Fiber Optic Dual Gooseneck
Microscope Illuminator
Figure 3
Headlight+Loupes
Flip Up Loupes
Fiber Optic Microscope
Ring Illuminator
Working distance
Day 1Surgical Instruments:• List of necessary instruments for mouse surgery• Care and cleaning, sterilization
Surgical Station:• Table (heated and non-heated)• Securing animals on the surgical table• Hair removal and preparation of surgical region
Microscopes:• Type of microscopes needed for the surgery• Lighting sources• Depth of field, field of vision
Acute and Chronic Surgery:• Aseptic technique, sterilization methods• Sutures and suturing techniques• Catheter material and manufacture
Anesthetics and Analgesics:• Types of anesthetic for surgery• Types of analgesics for chronic surgery• Postoperative care (chronic procedures)• Respirators and ventilators for anesthesia
Sterilization
• Sterilization can be achieved by1. Heat (autoclave)2. Chemicals3. Irradiation4. Filtration or combination
Hot Bead SterilizersFST. #18000-45
#18000-50
Daring the surgery day you can sterilize your surgical tools using hot bead sterilizer. Before sterilizing clean your tools with 70% ethanoland remove the blood from the tools
Sutures and suturing techniques• During the surgery never use big size needles and sutures, They can cause
severe damage of tissue and skin.For closing mouse skin use-6-0 or 5-0 Ethilon®, nylon suture w/ reverse cutting (C-2) needle.-6-0or 5-0 Vicryl®, polyglactin suture w/ taper (RB-1) needle.- You can also use any tupe 5-0 or 6-0 absorbable suturesFor mouse transaortic banding use5-0 or 6-0 non-absorbable sutures with or without needels. For LAD ligation, use 8-0 Ethilon®, nylon suture w/ taper (BV130-5) needle.For femoral and carotid artery, jugular vein isolation and catheterization use5-0 or 6-0 sutures.
FST. Castroviejo Needle Holder
#12565-14#12060-01
Always use small needle holder with or without lock
#18020-60
Catheters
During catheterization always pay attention on outer and inner dimmer of the catheter. Commonly used lab catheters diameters are shown in the figure below.
Day 1Surgical Instruments:• List of necessary instruments for mouse surgery• Care and cleaning, sterilization
Surgical Station:• Table (heated and non-heated)• Securing animals on the surgical table• Hair removal and preparation of surgical region
Microscopes:• Type of microscopes needed for the surgery• Lighting sources• Depth of field, field of vision
Acute and Chronic Surgery:• Aseptic technique, sterilization methods• Sutures and suturing techniques• Catheter material and manufacture
Anesthetics and Analgesics:• Types of anesthetic for surgery• Types of analgesics for chronic surgery• Postoperative care (chronic procedures)• Respirators and ventilators for anesthesia
Mouse anestheticsInjectable anesthetics: ketamine/Xilazine (intraperitoneal injection) ; 10/1 ration is commonly used anesthetic for long term mouse surgery. If surgery takes >30 minutes, another extra dose will be administered. The other alternative to keep animals anesthetized after injection is gas(Isoflurane) anesthesia (1-2% with 100% oxygen)For short term procedures gas anesthesia can be used(isoflurane 2-3% with 100 % oxygen through nose cone).
Intraperitoneal injection
Isoflurane 3-4%= HR = 350-300
Isoflurane 1.5-2.5% HR= 550-450
kv 1.5 #138
Ch
1, B
P (m
mH
g)
-200
-100
0
100
200
hx
21:00 21:10 21:20 21:30 21:40 21:50 22:00 22:10 22:20 22:30 22:40 22:50 23:00 23:10 23:20 23:30 23:40 23:50 24:00 24:10 24:20 24:30 24:40 24:501
12:20:54.200 AM
Signs of adequate anesthesia• Adequate general anesthesia is accompanied by loss of muscle tone reflected in loss of purposeful
movements. There is loss of reflexes for example corneal, pinnae and pedal. There should be no response to aversive stimuli e.g. tail pinch, pinching abdominal skin with forceps and a lack of vocalization. There are changes in the depth and frequency of respiration and cardiovascular parameters.
Monitoring the depth of anesthesia• Assess movement, stimulus perception and reflexes - [cornea, toe, tail or ear]
• Observe chest wall movement
• Pulse, heart rate, direct or indirect blood pressure (cuff or Doppler)
• Temperature
Analgesics
• Buprenorphine (0.05-0.1 mg/kg)
Inject one dose before the surgery. Inject second and third doses of Buprenorphine (0.05-0.1 mg/kg) 12 and 24 hours after the operation (12 hours intervals).
Bupivacaine(0.2cc)
0.2cc of diluted bupivacaine [0.025%] (diluted stock 1/10 with sterile saline) around the surgical area.
After administration of this analgesics, mouse will be ready for the surgery.
Ventilators and anesthesia stations
Harvard apparatusKent Scientific
Nose cones
Video
• For more information, please visit our websites:
• http://www.neomed.edu/academics/medicine/departments/integrative-medical-sciences/microecho
• https://www.facebook.com/pages/Mouse-Microsurgery-and-Echocardiography-Workshop/398774443577599