Isothesia

Name: Isothesia
Brand: Henry Schein
SKU: UiXhCZIBPBHhf-iF_rNu
Availability: InStock

Manufactured by Henry Schein

69 citations

Sourced in United States, Australia, Ireland, United Kingdom

About the product

Isothesia is a lab equipment product designed for temperature control and analysis. It maintains a stable and precise temperature environment for various laboratory applications.

Automatically generated - may contain errors

Get Technical Specifications Find protocols

Market Availability & Pricing

The isothesia product details are unclear. While it may have been previously available, we could not confirm if it is still commercialized by the manufacturer or if it has been discontinued. No official replacement model was identified. As this product's status is uncertain, we recommend contacting Henry Schein directly for the most up-to-date information.

Need Operating Instructions, SDS, or distributor details? Just ask our AI Agent.

Is this product still available?

Get pricing insights and sourcing options

Lab products found in correlation

Metacam, by Boehringer Ingelheim (6 mentions) Teets, by Patterson Dental (5 mentions) Aceproject, by Henry Schein (3 mentions) Der p 1, by Stallergenes Greer (2 mentions) Propoflo 28, by Abbott (2 mentions) Dexdomitor, by Zoetis (2 mentions) Vero cell, by American Type Culture Collection (2 mentions) Fetal bovine serum (fbs), by Atlanta Biologicals (2 mentions) Medroxyprogesterone acetate, by Sicor Pharmaceuticals (2 mentions) Infusion pump, by Harvard Apparatus (2 mentions) Cerulein, by Merck Group (2 mentions) Combi pen 48, by Henry Schein (2 mentions) Dextrose, by Baxter (2 mentions) Digital stereotaxic frame, by Kopf Instruments (2 mentions) Legato 100 syringe pump, by KD Scientific (2 mentions) Pc sam small animal monitor, by SA Instruments (2 mentions) Ilium medetomidine injection, by Troy Laboratories (2 mentions) 4 6 diamidino 2 phenylindole (dapi), by Thermo Fisher Scientific (2 mentions) Enrofloxacin, by Norbrook (1 mentions) Enroflox, by Norbrook (1 mentions)

Check compatibility

69 protocols using «isothesia»

Unilateral 6-OHDA Lesion in Mice

2025

Before surgery, mice were acclimatized in the housing facilities for at least a week. Mice were randomized into treatment groups based on their body weight and sex. Differences in the average body weight between groups were less than 1.5 grams. Groups of 4 or 5 mice were housed per cage to ensure even distribution of vehicle- and 6-OHDA-infused mice within the same cage. To reduce stress levels, mice were handled for 4 days before surgical procedures. Mice were anesthetized using 4% isoflurane (Isothesia, Henry Schein Animal Health, Dublin, OH) in a mixture of oxygen and compressed air. The toe pinch reflex confirmed full anesthetic induction. Immediately after induction, mice received a subcutaneous (s.c.) injection of USP solution (10 mL/kg) with 5% dextrose (Baxter, Deerfield, IL) and 1 mg/kg Buprenorphine SR LAB (ZooPharm). Mice were shaved on top of the skull and positioned on a digital stereotaxic frame (David Kopf Instruments), with isoflurane maintained at 1.5–2% throughout the surgery. Eye drops were applied to keep the cornea moisturized, and the skull surface was disinfected 3X with Betadine and 70% ethanol solution. An 8 mm median incision above the skull was topically anesthetized twice with 5 mg/mL lidocaine (Xylocain MPF, Fresenius Kabi, USA). Respiration rate, skin color, and toe-pinch reflex were monitored every 15 min, while normothermia was maintained through a heating pad (WPI, ATC2000) connected to a feedback loop rectal probe (WPI). After intracranial convection-enhanced delivery (CED) of 6-OHDA or vehicle, mice were placed in recovery cages and kept warm with heating pads, with free access to 98% water hydrogel (Clear H₂O) for approximately 5 h before returning to their home cage. Saline was administered s.c. every day for 5 consecutive days, with wetted food provided throughout the treatment period. Buprenorphine SR LAB was administered every 48 h to manage pain. Attrition rates ranged between 5 and 30% depending on the sex and dose of 6-OHDA infused. Pre- and post-surgical care was conducted per the guidelines outlined by Masini et al.^{11 (link)}.
6-OHDA hydrochloride was from Sigma Aldrich (Cat: H4381 Lot number: MKCG8789). 6-OHDA handling and infusions were carried out following the guidelines and safety procedures described by Stott and Barker^{18 (link)}. Using convection-enhanced delivery (CED), 6-OHDA was infused at one of three dosages: 5 µg (low dose)^{35 (link)}, 10 µg (medium dose)^{18 (link)}, or 20 µg (high dose)^{17 (link)}. Vehicle control mice were infused with USP saline 0.9% containing 0.03% ascorbic acid. Mice were unilaterally infused at a rate of 0.5 μL/min into the dorsal striatum (AP = +0.5 mm, ML = +2.1 mm, DV = −3.20 mm from bregma (see Fig. 1A)). The equipment used for CED consisted of a 10 µL airtight syringe (Hamilton), a 33-gauge Hamilton needle, and a microinjection pump (UMP3, WPI) connected to an intelligent touch controller (WPI). After the infusion, the needle was left in place for 5 min before being slowly withdrawn. The incision site was closed with tissue adhesive (3 M Vetbond Tissue Adhesive, Cat: 1469SB). Before every infusion, the needle and syringe were inspected to ensure accurate delivery of a total volume of 2 µL.

Santoro M., Lam R.K., Blumenfeld S.E., Tan W., Ciari P., Chu E.K., Saw N.L., Rijsketic D.R., Lin J.S., Heifets B.D, & Shamloo M. (2025). Mapping of catecholaminergic denervation, neurodegeneration, and inflammation in 6-OHDA-treated Parkinson’s disease mice. NPJ Parkinson's Disease, 11, 28.

+ Open protocol

+ Expand

6-OHDA Mouse Model of Parkinson's Disease

2024

Santoro M., Lam R.K., Blumenfeld S.E., Tan W., Ciari P., Chu E.K., Saw N.L., Rijsketic D.R., Lin J.S., Heifets B.D, & Shamloo M. (2024). Mapping of catecholaminergic denervation, neurodegeneration, and inflammation in 6-OHDA-treated Parkinson’s disease mice. Research Square.

+ Open protocol

+ Expand

Co-infection Dynamics of SARS-CoV-2 and Enteroviruses

2024

Co-infection with SARS-CoV-2 and LEV-8 or EV-A71 was studied using Syrian hamsters. The animals were randomly assigned to multiple groups (n = 9 animals per group). The Syrian hamsters were intranasally challenged with SARS-CoV-2 (10⁵ TCID₅₀), or challenged with SARS-CoV-2 (10⁵ TCID₅₀) and LEV-8 (10⁶ TCID₅₀); another group of animals were intranasally challenged with LEV-8 (10⁶ TCID₅₀), and, on Day 3, they were challenged with SARS-CoV-2 (10⁵ TCID₅₀). Furthermore, the Syrian hamsters were simultaneously intranasally challenged with SARS-CoV-2 (10⁵ TCID₅₀) and EV-A71 (10⁶ TCID₅₀). The pre-infection with EV-A71/3 days/SARS-CoV-2 was similar to that performed using 10⁶ TCID₅₀ EV-A71. Intranasal inoculation was performed by anesthetizing the hamsters with isoflurane (Isothesia; Henry Schein Animal Health) and then inoculating the nostrils with the viruses in 150 µL of phosphate-buffered saline (PBS). The control animals received PBS alone. After challenge, the hamsters were followed up and weighed daily. On Day 4 and Day 7 post-infection (for the LEV-8/3 days/SARS-CoV-2 and EV-A71/3 days/SARS-CoV-2 groups, this took place on Day 4 and Day 7 after the challenge with SARS-CoV-2), the lungs were collected from three hamsters from each group. Animal euthanasia was carried out using an automated compact CO₂ system for humane output from the experiment of laboratory animals (Euthanizer, Moscow, Russia). The concentration of carbon dioxide (30% at the 1st stage, 70% at the 2nd stage) and the gas supply rate met the requirements of the American Veterinary Medical Association, 2020. The lung tissues were homogenized and used to determine the infectious titers of the viruses and viral RNA loads. The SARS-CoV-2 and LEV-8 or EV-A71 titers, expressed as the TCID₅₀, were determined using the cytopathic effect (CPE) assay in the Vero E6 and HEK293A cells, respectively. The lung homogenates were analyzed for viral genome load via digital polymerase chain reaction (dPCR). The SARS-CoV-2, LEV-8, and EV-A71 viral genome loads were determined using primers targeting the 1ab, 2C, and 5′UTR sequence, respectively. On Day 7 post-infection, the lung tissues from three animals were fixed in formalin and used for the pathohistological study [16 (link)]. The slides were stained using the standard hematoxylin–eosin staining procedure. Optical microscopy and microphotography were carried out using an Imager Z1 microscope (Zeiss, Göttingen, Germany) equipped with a high-resolution HRc camera. The images were analyzed using the AxioVision Rel.4.8.2 software package (Carl Zeiss MicroImaging GmbH, Jena, Germany).

Svyatchenko V.A., Legostaev S.S., Lutkovskiy R.Y., Protopopova E.V., Ponomareva E.P., Omigov V.V., Taranov O.S., Ternovoi V.A., Agafonov A.P, & Loktev V.B. (2024). Coxsackievirus A7 and Enterovirus A71 Significantly Reduce SARS-CoV-2 Infection in Cell and Animal Models. Viruses, 16(6), 909.

+ Open protocol

+ Expand

LPS-Induced Endotoxemia in WT and α7nAChR Mice

2024

In survival experiments, male or female WT and α7nAChR^−/− mice were intraperitoneally injected with a sublethal dose of LPS calculated based on body weight. Since LPS activity is slightly variable from bath to bath, we evaluated the sublethal dose for each vial preparation using increasing doses of LPS (E. coli O55:B5) in C57BL/6J wild-type mice. Female mice are more resistant to LPS treatment compared to male mice [24 (link), 25 (link)]. Therefore, a gender-specific dosing was applied to reach a similar percentage of lethality for male and female mice. Depending on the LPS bath preparation we used 7–8 mg/kg for males and 9–12 mg/kg for females. Notably, the same concentration of LPS was used for all groups in each experiment.
In all endotoxemia experiments, body temperature was monitored twice daily using a rectal probe connected to a ThermoWorks (American Fork, UT, USA) MicroTherma meter.
To examine macrophage accumulation in the lungs, male or female WT and α7nAChR^−/− mice were given an intraperitoneal injection of LPS as described above. After 48h, mice were euthanized using Isothesia (Henry Schein Animal Health, Dublin, OH) and perfused, and lungs were removed. Lungs were digested using collagenase II as described below ( "Flow Cytometry and Imaging Flow Cytometry Analyses" section) and prepared for flow cytometry. In an additional experiment, male and female WT mice were treated intraperitoneally with 3mg/kg PNU-282987, 15 min before the injection of LPS, to examine the effect of α7nAChR stimulation on macrophage accumulation. Control mice received DMSO (vehicle) 15 min before LPS. Samples were incubated with anti-αM/PE-Cy7, anti-CCR2/APC, anti-CCR5/PE-Cy7, anti-Siglec F/FITC, anti-Ly6-G/PE, anti-F4/80/PE, anti-F4/80/APC, and anti-αX/APC across multiple samples.

Keever K.R., Cui K., Casteel J.L., Singh S., Hoover D.B., Williams D.L., Pavlov V.A, & Yakubenko V.P. (2024). Cholinergic signaling via the α7 nicotinic acetylcholine receptor regulates the migration of monocyte-derived macrophages during acute inflammation. Journal of Neuroinflammation, 21, 3.

+ Open protocol

+ Expand

Corresponding organizations : East Tennessee State University, Feinstein Institute for Medical Research, Northwell Health

Viral Coinfection Dynamics in Hamsters

2023

SARS-CoV-2 and HAdV-5 coinfection was studied in vivo using Syrian hamsters. The animals were randomly assigned to multiple groups (n = 9 animals per group): “CoV” (SARS-CoV-2)—on Day 0, the Syrian hamsters were intranasally challenged with SARS-CoV-2 (10⁵ TCID₅₀); “CoV/ad” (SARS-CoV-2/HAdV5)—on Day 0, the Syrian hamsters were simultaneously intranasally challenged with SARS-CoV-2 (10⁵ TCID₅₀) and HAdV-5 (10⁶ TCID₅₀); “ad/3-days/CoV”—on Day 0, the hamsters were intranasally challenged with HAdV-5 (10⁶ TCID₅₀), and, on Day 3, they were challenged with SARS-CoV-2 (10⁵ TCID₅₀); “ad”(HAdV5)—on Day 0, the Syrian hamsters were intranasally challenged with HAdV-5 (10⁶ TCID₅₀); “control”—mock-infected animals. Intranasal inoculation was performed by anaesthetizing the hamsters with isoflurane (Isothesia; Henry Schein Animal Health) and then inoculating the nostrils with the viruses in 150 µL of phosphate buffered saline (PBS). The control animals were administered PBS. After challenge, the hamsters were observed and weighed daily. On Day 4 postinfection (for the ad/3-days/CoV group, this took place on Day 4 after the challenge with SARS-CoV-2), the lungs were collected from three hamsters from each group. The lung tissues were homogenized and used to determine the infectious titers of the viruses and viral RNA/DNA loads. The SARS-CoV-2 and HAdV-5 titers, expressed as the 50% tissue culture infectious doses (TCID₅₀), were determined by the cytopathic effect (CPE) assay in Vero E6 and HEK293A cells, respectively. The lung homogenates were analyzed for viral genome load by digital polymerase chain reaction (dPCR). The SARS-CoV-2 and HAdV-5 viral genome loads were determined using primers targeting the 1ab and hexon genes, respectively. On Day 6 postinfection (for the group ad/3 days/CoV, this took place on Day 6 after the challenge with SARS-CoV-2), the lung tissues from three hamsters were fixed in formalin and used for the pathohistological study [18 (link)]. The slide samples were stained using a standard hematoxylin–eosin staining procedure. Light-optical examination and microphotography were carried out using an Imager Z1 microscope (Zeiss, Göttingen, Germany) equipped with a high-resolution HRc camera. The images were analyzed using the AxioVision Rel.4.8.2 software package (Carl Zeiss MicroImaging GmbH, Jena, Germany).
Coinfection with SARS-CoV-2 and IAV was studied in both ferret and hamster models. On Day 0, ferrets and hamsters were intranasally infected with 10² TCID₅₀ and 2 × 10³ TCID₅₀ of IAV, respectively. Then, the ferret (on Day 2) and hamster (Day 4) groups were intranasally infected with 3 × 10⁵ TCID₅₀ and 10⁴ TCID₅₀ of SARS-CoV-2, respectively. After the challenge, the animals were observed and weighed daily. On Days 6, 8, and 10 after infection with IAV for the hamsters and on Days 4, 6, and 8 after infection with IAV for the ferrets, nasopharyngeal wash samples were collected from the animals to determine the viral genome loads. Animals were anaesthetized with intramuscular injection of tiletamine/zolazepam (Zoletil 100, Delpharm Tours, Chambray-lès-Tours, France) + xylazine (Xila, Interchemie, Venray, Estonia) at a dose of 30 + 10 mg/kg for hamsters and 5 + 3 mg/kg for ferrets; nasopharyngeal washes in ferrets and hamsters were obtained by administering 500 µL and 100 µL PBS to each nostril, respectively. On Day 10 post-monoinfection with IAV or on Day 10 postinfection with IAV and Day 6 postinfection with SARS-CoV-2 for the double-infected animals, the lungs were collected from the hamsters, and the lung tissues were fixed in formalin and used for the pathohistological study. Animal euthanasia was carried out using an automated compact CO₂ system for humane output from the experiment of laboratory animals (Euthanizer, Moscow, Russia). The concentration of carbon dioxide (30% at the 1st stage, 70% at the 2nd stage) and gas supply rate satisfy the requirements of the American Veterinary Medical Association (AVMA) 2020.

Svyatchenko V.A., Ternovoi V.A., Lutkovskiy R.Y., Protopopova E.V., Gudymo A.S., Danilchenko N.V., Susloparov I.M., Kolosova N.P., Ryzhikov A.B., Taranov O.S., Omigov V.V., Gavrilova E.V., Agafonov A.P., Maksyutov R.A, & Loktev V.B. (2023). Human Adenovirus and Influenza A Virus Exacerbate SARS-CoV-2 Infection in Animal Models. Microorganisms, 11(1), 180.

+ Open protocol

+ Expand

Corresponding organizations : State Research Center of Virology and Biotechnology VECTOR

Top 5 most cited protocols using «isothesia»

Ventral Hippocampus Modulates Fear Discrimination

Cited 8 times

Sixteen adult male Sprague-Dawley rats were obtained from Charles River Labs (Wilmington, MA) weighing 250–300 g upon arrival. Rats were housed individually in plastic tub cages with free access to food and water and a short length of autoclaved manzanita wood for enrichment in the Boston College Animal Care Facility. The vivarium maintained a 12 h light/dark cycle. All rats were allowed to acclimate to the colony housing for 7 days prior to surgery. All experimental protocols were reviewed and approved by the Boston College Institutional Animal Care and Use Committee.
Under isoflurane anesthesia (3% in O², Isothesia, Henry Schein, Dublin, OH) in a stereotaxic frame, as previously (3 (link)), stainless steel guide cannulae (22 g; Plastics One, Roanoke, VA) were implanted to target the VH as in (13 (link)) at −5.8 mm posterior to bregma, ±5.2 mm from midline, and −7.0 mm ventral to the surface of the skull. A stylet was placed in each cannula, which extended 1 mm below the tip of the guide. Immediately after surgery, each rat received loxicom (1mg/kg, Eloxiject, Henry Schein) and penicillin G procaine (15,000 Units, Combi-Pen-48, Henry Schein). Behavioral testing began 7–10 days after surgery.
Microinjections were made by gently restraining the rat in a cloth towel. Stylets were removed and replaced with a microinjector that extended 1 mm beyond cannula tip (33g; Plastics One). Each rat was injected bilaterally with 1 μL of either muscimol (Sigma, St. Louis, MO) in saline (1 μg per side) or saline alone at a rate of 1 μL/min. Injectors were left in place for an additional minute to allow for diffusion. The concentration was equal to that used by Hobin et al. (13 (link)). Injections were made 1 h prior to behavioral treatments as previously (16 (link)).
Fear conditioning occurred in chambers made of black plastic with wire mesh lids 10 x 11 x 6-in (L x W x H) with a stainless steel shock grid (Model H10-11R-TC-SF, Coulbourn Instruments, Whitehall, PA) enclosed within a 15 x 12 x 27-in (L x W x H) ventilated light and sound-attenuating chamber. Two infrared LED arrays (CMVision Model IR30) illuminated the chamber, and overhead cameras (Model VX-5000, Microsoft, Redmond, WA) with the manufacture’s infrared blocking filters replaced with infrared passing filters allowed for automated freezing detection with ANY-Maze software (version 4.99, Stoelting, Wood Dale, IL) as previously (17 (link)). Stimuli were delivered by a white LED array (Model LPL620WTHD, Hampton Bay) and speaker mounted at the top of the enclosure; a ventilation fan provided masking noise at ~55dB. The conditioning stimuli were a flickering white LED light (264.0 Lux, 20ms on/off) and a white noise pip (pip duration = 10ms, interval = 3 Hz, 75dB). Assignment of light or pip to CS+ or CS− was counterbalanced. No effect of the cue stimulus was evident as both the light and pip produced equivalent fear conditioning and discrimination behavior (data not shown).
To begin conditioning, rats were transferred from the vivarium, placed in the apparatus, and conditioning trials began immediately. Conditioning trials lasted 90 seconds beginning with a 70 s blackout (inter-trial-interval) after which a 5 s, 1 kHz tone (75dB) signaled the upcoming CS presentation. Then, either the CS+ cue or the CS− cue was administered for 15 seconds. CS+ trials concluded with a 500 ms, 1 mA shock (Model H13-15, Coulbourn Instruments). Training consisted of 15 trials of each cue presented in quasi-randomized order so that one trial type never occurred more than 2 times in series. Recall tests began by placing the rat in the conditioning apparatus. After 2 minutes rats received 6, 1 min presentations of each the CS+, the CS− or the context alone in a quasi-random order.
A schematic diagram of the procedures is provided in Figure 1. On day 1, rats were randomly assigned to either muscimol or vehicle conditions, injected and returned to the homecage. 1 h later all rats received CS+/CS− conditioning. Fear recall and discrimination were assessed on Days 2 and 3 in identical tests. To test the role of VH in fear discrimination recall, all rats received additional conditioning and testing until both the vehicle and muscimol treated rats exhibited equal fear and discrimination. This required two additional drug-free CS+/CS− training sessions, which began in the afternoon on Day 3 and again on Day 4. Recall tests were given on the morning of Day 4 and Day 5 at which point all rats exhibited equal freezing and discrimination, regardless of past drug treatment. Rats were then assigned to new muscimol and vehicle groups each consisting of 4 rats from the previous muscimol group and 4 rats from the previous vehicle group. To test the role of VH in fear discrimination recall, on day 8 rats received either muscimol or vehicle, according to their new groups and 1 h later given a final recall test.
At the conclusion of the experiment rats were overdosed with tribromoethanol (Sigma), sacrificed and brains were flash frozen in 2-methylbutane on dry ice. Sections (40 μm) containing the ventral hippocampus were stained with cresyl violet and cannula placement was determined by comparison to the Rat Brain Atlas in Stereotaxic Coordinates (Paxinos and Watson, 2006). Only rats with cannula located in the ventral hippocampus were used in the statistical analysis (Figure 2).

Chen V.M., Foilb A.R, & Christianson J.P. (2015). Inactivation of ventral hippocampus interfered with cued-fear acquisition but did not influence later recall or discrimination. Behavioural brain research, 296, 249-253.

+ Open protocol

+ Expand

Corresponding organizations : Boston College

Evaluating Murine Models of Herpes Simplex Virus Infection

Cited 4 times

Mice were treated with MPA and challenged 5 days later with HSV-2(4674) 3 weeks after the vaccine boosting dose with 5 × 10⁴ plaque forming units (pfu, LD₉₀) or 5 × 10⁵ pfu (10× LD₉₀) of HSV-2(4674) intravaginally and monitored and scored for disease for 14 days as previously described (Nixon et al., 2013 (link)). For safety studies, unimmunized SCID mice were treated with MPA and inoculated 5 days later intravaginally or subcutaneously with HSV-2 (4674) or ΔgD^−/+gD−1 either with 30 µl or 100 µl total volume, respectively. 150 µl of sterile PBS containing protease inhibitor (F Hoffmann-La Roche AG, Switzerland) was used to perform intravaginal washes for antibody and viral load quantification. Epithelial disease for intravaginal infections was scored as follows: (1) mild erythema, (2) hair loss, erythema, edema, (3) severe edema, hair loss, lesion formation, (4) severe ulcerations, multiple lesions and (5) death. Neurological disease for intravaginal infection was scored as follows: (1) urinary retention, (2) urinary retention and constipation, hind-limp paresis, (3) hind-limb paralysis (one leg), (4) complete hind limb paralysis (both legs), and (5) death. Mice were euthanized at a score of 3 or 4 and assigned a score of 5 on subsequent days for statistical analyses. For HSV skin infections, a protocol modified from Goel et al. (2002) (link) was used. Briefly, mice were depilated on the right flank with Nair and allowed to rest for 24 hr. Depilated mice were anesthetized with isoflurane (Isothesia, Henry-Schein), then abraded on the exposed skin with a disposable emory board for 20–25 strokes and subsequently challenged with 5 × 10⁴ pfu of HSV-2(4674) or 1 × 10⁷ pfu of HSV-1(17) in 5 µl deposited on the abraded skin. Mice were then anesthetized for an additional 5 min to allow the virus inoculum to dry. Mice were monitored for 14 days and scored for signs of disease. Epithelial disease in the skin scarification model was scored as follows: (1) primary lesion or erythema, (2) distant site zosteriform lesions, mild edema/erythema, (3) severe ulceration and edema, increased epidermal spread, (4) hind-limb paralysis and (5) death. Mice that were euthanized at a score of 4 were given a value of 5 the next day.

Petro C., González P.A., Cheshenko N., Jandl T., Khajoueinejad N., Bénard A., Sengupta M., Herold B.C, & Jacobs WR J.r. (2015). Herpes simplex type 2 virus deleted in glycoprotein D protects against vaginal, skin and neural disease. eLife, 4, e06054.

+ Open protocol

+ Expand

Corresponding organizations : Albert Einstein College of Medicine, Howard Hughes Medical Institute, Millennium Institute on Immunology and Immunotherapy, Pontificia Universidad Católica de Chile

Targeted Insular Cortex Manipulation in Rats

Cited 3 times

Surgical procedures and cannula placements were conducted as previously described (Christianson et al., 2011 (link); Chen et al., 2015 (link)). Rats were anesthetized with isoflurane (3% in oxygen; Isothesia, Henry Schein, Dublin, OH) and placed in a stereotaxic apparatus. Stainless steel guide cannula (22 g; Plastics One, Roanoke, VA) were implanted bilaterally to target anterior (AP +2.7, ML ±3.9, DV −5.2), medial (AP +0.5, ML ±4.9, DV −6.2), or posterior (AP −1.8, ML ±6.5, DV − 6.2) insular cortex. All coordinate measures (mm) were taken from the skull surface at bregma. The IC can be subdivided into granular, dysgranular and agranular regions along its dorsal-ventral axis. Here, cannula were targeted for the central agranular region and the injection volume (0.5μL) was selected to permit diffusion throughout the three regions. Cannula tips found within any of the three subdivisions were included, thus conclusions from these were not intended to be specific to any of the IC subregions. Cannula were fixed to the skull with stainless steel screws and acrylic cement and a stylet extending 1mm below the tip of the guide was placed in the cannula. Rats were given 1 mg/kg Loxicom (Eloxiject, Henry Schein) and penicillin (15,000 Units, Combi-Pen-48, Henry Schein) after surgery. A minimum of 7 days of recovery were allotted before behavioral testing, during which time rats were periodically handled and stylets were checked to ensure the cannula remained unobstructed. Microinjections were made by gently restraining the rat in a cloth towel and replacing the stylet with a microinjector connected with PE-50 tubing to a 25 μL syringe (Hamilton, Reno, NV) in a micromanipulator (Model 5000, Kopf Instruments, Tujunga, CA). The injector protruded 1 mm beyond the cannula tip (33g; Plastics One, Roanoke, VA). NMDArs were blocked with receptor antagonist D-(−)-2-Amino-5-phosphonopentanoic acid (AP5). AP5 (Tocris, Minneapolis, MN) was dissolved in sterile saline at 6 μg/μL (as in (Bast et al., 2005 (link); Amat et al., 2014 (link); Christianson et al., 2014 (link)). The GABA_A agonist muscimol was used to temporarily inactivate IC. Muscimol (Sigma, St. Louis, MO) was dissolved in sterile saline at 100 ng/μL (Moscarello and LeDoux, 2013 (link)). Each drug was administered bilaterally at 0.5 μL per side at a rate of 1 μL/min, with an additional minute allowed for diffusion. Vehicle treated animals received saline injections at the same volume and rate as the drug infusions. AP5 injections were completed 15 minutes before conditioning (Bast et al., 2005 (link)) and muscimol injections were completed an hour before testing (Amat et al., 2005 (link)). At the end of each experiment, rats were overdosed with tribromoethanol (Sigma, St. Louis, MO). Brains were removed and flash-frozen in 2-methylbutane on dry ice, and stored at −80°C until they were sliced at 40 μm on a freezing cryostat (−20°C). Slices were stained with cresyl violet, coverslipped, and allowed to dry overnight before cannula placement was determined by comparison with the Rat Brain Atlas in Stereotaxic Coordinates (Paxinos and Watson, 2007 ). Data from rats for which cannulas were not found or were located outside of the targeted areas of IC were excluded in statistical analysis (see Figure 2).

Foilb A.R., Flyer-Adams J.G., Maier S.F, & Christianson J.P. (2016). Posterior insular cortex is necessary for conditioned inhibition of fear. Neurobiology of learning and memory, 134(Pt B), 317-327.

+ Open protocol

+ Expand

Corresponding organizations : Boston College, University of Colorado Boulder

Medetomidine Dosing for Rodent Brain fMRI

Cited 2 times

The rats were randomly allocated to three experimental groups: Group T for determination of the target serum concentration of medetomidine when administered with low dose isoflurane for rodent brain fMRI studies (n = 8); Groups IV and SC for determination of the SC bioavailability of medetomidine during isoflurane anaesthesia (n = 8 each).
On the days of the procedures, the rats were anaesthetised with isoflurane (Isothesia™, Henry Schein Animal Health, 2000, Australia) in an induction chamber (4% isoflurane in 100% medical oxygen, 2 L/min). Once adequately anaesthetised (recumbent, no response to toe pinch) the rats were transferred onto the experimental benchtop and positioned for delivery of isoflurane throughout the experiment (0.5–2% isoflurane vapouriser setting in 100% medical oxygen, 1.5 L/min, Darvall Zero Dead Space face mask circuit, Advanced Anaesthesia Specialists) under a heat lamp. Physiological monitoring included body temperature, respiratory rate, heart rate, electrocardiography (PC-SAM Small Animal Monitor, SA Instruments Inc., 1030 System), exhaled isoflurane and CO₂ (data not shown) (ISATM Sidestream Gas Analyzer, Masimo Sweden AB and PHASEIN and Lightning Multi-Parameter Monitor Vetronic Services Ltd., Newton Abbot, UK) and blood glucose concentration (Accu-Chek Guide, Roche, Mannheim, Germany). These variables were recorded every 5 min. A single rat was studied at any one time, during the hours of 8 a.m. and 6 p.m.
Medetomidine (1 mg/mL, Ilium Medetomidine Injection, Troy Laboratories Pty. Limited, Glendenning, Australia) was administered according to the treatment group. In Group T, rats were administered an initial dose of medetomidine of 0.05 mg/kg SC over 1 s via a 29 G insulin syringe (BD Ultra-Fine Insulin Syringe, Becton Dickinson Pty Ltd., Macquarie University Research Park North Ryde, Australia), immediately followed by a continuous medetomidine infusion of 0.15 mg/kg/h SC, administered via a 25 G butterfly catheter connected to a single syringe infusion pump (Legato 100 Syringe Pump, KD Scientific Inc., Holliston, MA, USA). This protocol was developed empirically and used in our laboratory [10 (link)]. In the IV and SC groups, rats were manually administered a single dose of either IV (through a catheter placed in a lateral tail vein) or SC (under the skin over a flank) medetomidine at 0.05 mg/kg. The concentration of isoflurane was immediately reduced to 0.5% after administration of the initial dose of medetomidine and then subsequently altered to maintain an adequate depth of anaesthesia as assessed by response to toe pinch, heart rate and respiratory rate.
For serial blood sampling, a catheter was placed in the lateral tail vein (22 G, 1 IN, BD Angiocath IV Catheter, BD Australia, Seven Hills, NSW, Australia), secured with surgical tape and flushed with heparinised saline (5 IU/mL). In Group T, blood samples were collected 60 and 90 min after the initial dose of medetomidine. The conditions during anaesthesia were consistent with those observed in previous studies performed in this laboratory and were considered suitable for identification of the target concentration of medetomidine. In the IV group, blood was collected before medetomidine administration and 2, 5, 10, 20, 30, 60, 120 and 180 min afterwards. In the SC group, blood was collected before medetomidine administration and 10, 20, 30, 40, 50, 60, 120, 180 and 240 min afterwards. Following collection of the final sample, but before recovery from anaesthesia, the rats were euthanised via an intraperitoneal or IV injection of pentobarbitone (160 mg/kg, Lethabarb, Jurox, Rutherford, Australia).

Kint L.T., Seewoo B.J., Hyndman T.H., Clarke M.W., Edwards S.H., Rodger J., Feindel K.W, & Musk G.C. (2020). The Pharmacokinetics of Medetomidine Administered Subcutaneously during Isoflurane Anaesthesia in Sprague-Dawley Rats. Animals : an Open Access Journal from MDPI, 10(6), 1050.

+ Open protocol

+ Expand

Corresponding organizations : University of Western Australia, Perron Institute for Neurological and Translational Science, Murdoch University, Charles Sturt University

Tasmanian Devil Immunization and Sampling

Cited 2 times

The Tasmanian devils were housed in secured shelters in accordance with the guidelines of the Department of Primary Industries, Parks, Water and Environment of Tasmania (DPIPWE). All animal procedures were approved by the University of Tasmania Animal Ethics Committee under A009215, A0011436 and A0013685. All devils (6 females and 3 males) were adults with ages ranging from 5 to 7 years at commencement of experiments (Supplementary Table S5). All experimental methods were performed in accordance with the University of Tasmania guidelines.
Immunisation, blood collection, live cell challenge and therapy were performed under anaesthesia induced with 5% Isoflurane reducing to 3% via a mask (ISOTHESIA^® (Henry Schein, Northgate, Australia). 10 ml of blood was obtained from the jugular vein as previously described27 (link). Up to 4 ml of blood was placed into clot activating tubes (Greiner Bio-one) for serum analysis and the remainder into lithium heparin anticoagulant tubes for cell analyses. Tumour biopsies were collected using sterile 4 mm disposable biopsy punches (Kai Medical). Biopsies were divided with a scalpel blade and half placed into 1 ml 10% neutral buffered formalin and half into 1 ml RNAlater.

Tovar C., Pye R.J., Kreiss A., Cheng Y., Brown G.K., Darby J., Malley R.C., Siddle H.V., Skjødt K., Kaufman J., Silva A., Baz Morelli A., Papenfuss A.T., Corcoran L.M., Murphy J.M., Pearse M.J., Belov K., Lyons A.B, & Woods G.M. (2017). Regression of devil facial tumour disease following immunotherapy in immunised Tasmanian devils. Scientific Reports, 7, 43827.

+ Open protocol

+ Expand

Corresponding organizations : University of Tasmania, University of Sydney, University of Southampton, University of Southern Denmark, University of Cambridge, CSL (Australia), Walter and Eliza Hall Institute of Medical Research

Spelling variants (same manufacturer)

Isothesia NXT - 3 citations

Similar products (other manufacturers)

Isothesia (by Abbott) - 25 citations Isothesia (by Butler Animal Health Supply) - 14 citations IsoThesia (by Vetus Animal Health) - 12 citations Isothesia (by Fisher Biotech) - 7 citations

The spelling variants listed above correspond to different ways the product may be referred to in scientific literature.
These variants have been automatically detected by our extraction engine, which groups similar formulations based on semantic similarity.

About PubCompare

Our mission is to provide scientists with the largest repository of trustworthy protocols and intelligent analytical tools, thereby offering them extensive information to design robust protocols aimed at minimizing the risk of failures.

We believe that the most crucial aspect is to grant scientists access to a wide range of reliable sources and new useful tools that surpass human capabilities.

However, we trust in allowing scientists to determine how to construct their own protocols based on this information, as they are the experts in their field.

Ready to get started?

Revolutionizing how scientists
search and build protocols!