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Surgical microscope

Manufactured by Olympus
Sourced in Japan

The Olympus surgical microscope is a precision optical instrument designed for use in medical procedures. It provides a clear, magnified view of the surgical site, enabling healthcare professionals to perform delicate and intricate operations with enhanced visibility and precision.

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7 protocols using surgical microscope

1

Episcleral Vein Cauterization in Ocular Hypertensive Rats

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For comparison with ocular hypertensive rats, episcleral vein cauterization was performed. After intraperitoneal injection of 50 mg/kg ketamine with zolazepam (Zoletil; Virbac, Carros, France) and 15 mg/kg xylazine hydrochloride (Rompun, Bayer, Leverkusen, Germany), three episcleral veins were cauterized using a surgical microscope (Olympus, Tokyo, Japan). Retinal vascular perfusion was assessed using planar ophthalmoscopy after cauterization. IOP was measured using a Tono-pen (Solan, Florida, USA) after topical anesthetization with Alcaine (Alcon Laboratories, Fort Worth, Texas, USA).
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2

Inducing Neuropathic Pain in Rats via Sciatic Nerve Ligation

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For inducing neuropathic pain in animals, we used TST method. Rats were anesthetized using phentobarbital sodium (50 mg/kg), and the left sciatic nerve was exposed. Under a surgical microscope (Olympus, Tokyo, Japan), the three major divisions of the sciatic nerve (tibial, sural, and common peroneal nerves) were clearly separated. To generate an efficient neuropathic pain model, the tibial and sural nerves were completely ligated and transected except peroneal nerve. Hemostasis was completed and the cut was closed with muscle and skin sutures11) (link).
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3

Spared Nerve Injury Model for Neuropathic Pain

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To induce neuropathic pain, we used the spared nerve injury (SNI) method [18 (link)]. Rats were deeply anesthetized with pentobarbital sodium (50 mg/kg, intraperitoneally), and the left sciatic nerve was exposed. Under a surgical microscope (Olympus, Tokyo, Japan), the three major divisions of the sciatic nerve were exposed, and the common peroneal and tibial nerves were completely ligated and transected. Hemostasis was completed, and the cut was closed with muscle and skin sutures.
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4

Episcleral Vein Cauterization Protocol

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Anesthesia was performed by intraperitoneal injection of 50 mg/kg ketamine with zolazepam (Zoletil; Virbac, Carros, France) and 15 mg/kg xylazine hydrochloride (Rompun, Bayer, Leuverkeusen, Germany). Cautery of three episcleral veins were performed using a surgical microscope (Olympus, Tokyo, Japan). Then, normal perfusion of the retina was checked using planar ophthalmoscopy after cauterization. IOP was measured using a Tono-pen (Solan, Florida, USA) after topical anesthetization with Alcane (Alcon Laboratories, Fort Worth, Texas, USA). Eyes that did not present any complications during surgery or scleral burns were used.
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5

Elevated IOP Induction via Venous Cauterization

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Elevated IOP was induced via venous cauterization. Briefly, animals were anesthetized with a mixture of tiletamine plus zolazepam (Zoletil; Virbac, France)/xylazine hydrochloride (Rompun; Bayer, Germany) (50/15 mg/kg ip injection). Proparacaine (0.5% concentration) was topically eye-dropped. Three of four episcleral veins in the right-side eyeball were cauterized with a 30-gauge tip cautery (Bovie Medical Co., USA) under a surgical microscope (Olympus, Tokyo, Japan). Animals were grouped and cared for 1 and 3 days, and 1, 2, 4, and 8 weeks after operation. Twenty animals each were assigned for each experimental time point and, 15 animals for normal control and 5 animals for aged-matched control.
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6

Stem Cell Therapy for Nerve Injury

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All rats were anesthetized using an intraperitoneal (i.p.) administration of a mixture of medetomidine (0.15 mg/kg, i.p.; Domitor; Nippon Zenyaku Kogyo Co., Ltd., Fukushima, Japan), midazolam (2 mg/kg, i.p.; Dormicum Astellas Pharma Inc., Tokyo, Japan) and butorphanol (2.5 mg/kg, i.p: Vetporphale Meiji Seika Pharma CO., Ltd., Tokyo, Japan). Anesthetized rats were maintained at a constant temperature of 37 °C on a warming plate. The neck skin was shaved and opened under a surgical microscope (Olympus, Tokyo, Japan). The SLN was exposed bilaterally and injured with a vascular clip (60 g/mm2; NATSUME SEISAKUSHO Co Ltd., Tokyo, Japan) over a period of 30 min. The muscle and skin layers were closed with 4–0 Vicryl sutures (Ethicon Inc., Somerville, NJ). The animals were randomly assigned to the following four groups: (1) Sham: SLN exposure without any damage to the nerve tissue; (2) Injury: not injected; (3) DMEM (-): 1 ml DMEM (-)-injected into the tail vein for 10 s simultaneously with the SLN damage; (4) SHED-CM: 1 ml SHED-CM-injected into the tail vein for 10 s simultaneously with the SLN damage.
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7

Inducing Lymphedema in Rat Tails

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Post‐surgical lymphedema was induced in the tails of SD rats. The rats were anesthetized with sodium pentobarbital (50 mg kg−1 intraperitoneally). Next, 0.1 mL of 2% methylene blue solution was injected intradermally into the end of the rat tail. An annular incision was made at 13 cm from the end of the tail. The skin and subcutaneous tissue were removed, thus removing the superficial lymphatic network. The muscles, tendons, bones, and major blood vessels below the dermis were left untouched. A surgical microscope (Olympus, Japan) was used to visualize the two deep lymphatic vessels stained with methylene blue, and the vessels were sutured with 6–0 silk thread and cut. This study was approved by the Animal Ethics Committee of China. All methods were performed in accordance with the relevant guidelines and regulations.
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