Introduction
Principle
Mouse preparation and care prior to 18F-FDG PET imaging
Animal handling
Housing
Temperature
Blood glucose level and diet conditions
Anaesthesia
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Apply sterile unmedicated eye drops or ointment to prevent corneal damage and desiccation.
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Place the mouse in the induction chamber where it is initially anaesthetized and latch the lid.
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Set the vaporizer concentration between 4–5% + 0.8–1 L/min [51] until the mouse becomes immobile.
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Reduce the vaporizer setting to the appropriate level (1–3% + 0.8–1 L/min [51]) for a stable heart rate and blood pressure.
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The mouse should remain in the induction chamber for 3 to 5 min after initial anaesthetic induction before moving it to the PET instrument.
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Once the mouse is ready, transfer it from the induction chamber onto the bed of the PET camera with a breathing device and mask that supplies a constant flow of the anaesthetic gas, keeping the mouse safely anaesthetized during PET scanning.
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Note: if the animal has subclinical respiratory disease, resulting in hypoventilation and mild respiratory compromise, in the book entitled Biology and Medicine of Rabbits and Rodents, Harkness et al. [31] advised pre-oxygenation with 100% oxygen for 3 to 5 min prior to anaesthesia induction.
18F-FDG administration
V (mL/kg) | VMax (mL) | G |
---|---|---|
5 (bolus) 25 (slow) | 0.125 | 25–28 |
During 18F-FDG PET imaging
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Visual monitoring includes watching the respiration (classifies the character of breathing), the colour of mucous membrane and skin (oxygenation state: blue—poor oxygenation; pale—poor blood perfusion), and the general behaviour of the mouse [3].
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Electronic equipment available for small animal monitoring include rectal probe (body temperature, 36.5–38 °C), electrocardiogram (heart function and rate, 350–700 beats/min), small pneumatic pillow (respiration rate, 80–220 breaths/min), clip-on-sensors (pulse oximeter, 1.63–2.17 mL/g/h), cuff sensor (blood pressure, systolic: 133–160 mmHg; diastolic: 102–110 mmHg) [31, 32, 49].