Spring scissors

Manufactured by Fine Science Tools

Sourced in Canada

Spring scissors are a type of laboratory equipment designed to facilitate precise and controlled cutting of various materials. They feature a spring mechanism that provides consistent tension, allowing for smooth and effortless operation. The spring-loaded design helps maintain a steady hand, making them suitable for tasks that require accuracy and precision.

Automatically generated - may contain errors

Lab products found in correlation

Paraformaldehyde (pfa), by Electron Microscopy Sciences (4 mentions) Phosphate buffered saline (pbs), by Thermo Fisher Scientific (3 mentions) Dumont 5 forceps, by Fine Science Tools (3 mentions) Phosphate buffered saline (pbs), by Fine Science Tools (2 mentions) Al104 analytical balance, by Mettler Toledo (1 mentions) Sylgard medium, by Thermo Fisher Scientific (1 mentions) Surgical scissors, by Fine Science Tools (1 mentions) Vannas spring scissors, by Fine Science Tools (1 mentions) Smz645 stereo microscope, by Nikon (1 mentions) Phosphate buffered saline (pbs), by Electron Microscopy Sciences (1 mentions) Ms 222, by Merck Group (1 mentions) Fedratinib, by Selleck Chemicals (1 mentions) Co2 independent medium, by Thermo Fisher Scientific (1 mentions) Fetal bovine serum (fbs), by Euroclone (1 mentions) Alcian blue, by Thermo Fisher Scientific (1 mentions) Axiozoom, by Zeiss (1 mentions) Stemi 305, by Zeiss (1 mentions) Axiocam 503, by Zeiss (1 mentions) Orbis oy a622f dc, by Basler (1 mentions) Culture dish, by Corning (1 mentions)

15 protocols using spring scissors

Dissection and Morphometric Analysis of Cicada Wings

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During dissection, cicadas were first weighed on a scale (AL104 Analytical Balance, Mettler Toledo; resolution, 0.1 mg), and full-body weights were collected. Each of their wings (left/right forewings and hindwings) were then carefully removed by cutting with scissors (Fine Science Tools, spring scissors) and individually weighed. The left forewing was removed first and weighed, followed by the left hindwing, right forewing, and right hindwing. After dissection, cicadas were quickly wrapped in facial tissues (Kleenex), labeled, and placed back in the freezer. Wrapping cicadas in tissue allowed us to anesthetize them rapidly, limit hemolymph bleeding, damage that the cicada might do to itself, and allowed us to quickly label the cicada (at this point, cicadas could still crawl away unless gently restrained). Wings were arranged on black cardstock and photographed using a DSLR camera (Nikon D850) and macro lens (Sigma 180 mm), using a micro SD card (length, 14.99 mm) as a scale bar. Imaging was illuminated with LED lighting, which was chosen because it does not locally heat the air (or wings).

Salcedo M.K., Ellis T.E., Sáenz Á.S., Lu J., Worrell T., Madigan M.L, & Socha J.J. (2023). Transient use of hemolymph for hydraulic wing expansion in cicadas. Scientific Reports, 13, 6298.

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Drosophila Tibia Amputation and Nutrient Supplementation

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Amputation was performed on adult flies 2–7 days after eclosion. Flies were anesthetized with CO₂, placed under a dissection microscope, and tibia amputated using a spring scissors (Fine Science Tools, 91500-09) and superfine dissecting forceps (VWR, 82027-402). See Figure 4 for detailed description of the amputation plane. Recovering Drosophila were allocated randomly to vials with standard lab fly food (control) or standard lab fly food mixed with 1.7 mM L-Leucine (Sigma-Aldrich L8000), 1.7 mM L-Glutamine (Sigma-Aldrich G3126), and 33 μg/ml insulin (human recombinant, MP Biomedicals 0219390080). To introduce the nutrient supplements, the fly food was microwaved in short pulses, such that the topmost layer of the food was liquified. The supplements in aqueous stocks were then pipetted into this liquified layer. Food was allowed to re-set at 4°C for at least 20 min. New food was prepared fresh every 2 days, and flies were moved into freshly prepared treated food every 2 days, throughout the course of the 2- to 3-week experiment.

Abrams M.J., Tan F.H., Li Y., Basinger T., Heithe M.L., Sarma A., Lee I.T., Condiotte Z.J., Raffiee M., Dabiri J.O., Gold D.A, & Goentoro L. (2021). A conserved strategy for inducing appendage regeneration in moon jellyfish, Drosophila, and mice. eLife, 10, e65092.

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Diaphragm NMJ Analysis Post-SCI

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Animals were euthanized with ketamine (300 mg/kg), xylazine (15 mg/kg) and acepromazine (6 mg/kg) 5 weeks following SCI. The hemi-diaphragm was exposed laterally along the rib cage and then excised using spring scissors (Fine Science Tools, Foster City, CA), stretched flat, pinned down to Sylgard medium (Fisher Scientific, Pittsburgh, PA), and washed with PBS. Diaphragm was then fixed in 4% paraformaldehyde (Electron Microscopy Sciences) for 20 min, followed by a wash in PBS. Superficial fascia were then carefully removed from the surface of the diaphragm, and diaphragm muscles were processed for NMJ immunohistochemistry. After hemi-diaphragm was removed, animals were perfused with 0.9% saline solution, followed by 4% paraformaldehyde. Spinal cord and brain were dissected and post-fixed in 4% paraformaldehyde overnight at 4°C. The tissue was then washed with 0.1M phosphate buffer solution for 24 hours and cryoprotected with a 30% sucrose solution for 3 days. The cervical spinal cord was embedded in tissue freezing medium, flash frozen, and sectioned in transverse or sagittal orientations at 20 μm thickness.

Ghosh B., Nong J., Wang Z., Urban M.W., Heinsinger N.M., Trovillion V.A., Wright M.C., Lepore A.C, & Zhong Y. (2019). A hydrogel engineered to deliver minocycline locally to the injured cervical spinal cord protects respiratory neural circuitry and preserves diaphragm function. Neurobiology of disease, 127, 591-604.

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Dissection and Isolation of Lumbosacral DRGs

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Dissections were performed under a Nikon SMZ645 stereo microscope. Mice were euthanized by carbon dioxide inhalation followed by cervical dislocation. Mice were laid on the dorsal side and immobilized on a dissection pad. Skin covering the ventral thorax and abdomen was removed together with internal organs to fully expose the ventral spinal column using surgical scissors (Fine Science Tools, #14054-13), supported by tissue forceps (Fine Science Tools, #11021-12). Muscles covering ventral side of the spinal column were removed using Spring Scissors (Fine Science Tools, #15751-11) to expose the lumbosacral peripheral nerves. To expose the lumbosacral DRGs, the ventral vertebrae were removed using the aforementioned Spring Scissors, aided by Octagon forceps (Fine Science Tools, #11042-08) with care taken not to sever nerves. DRGs were gently picked starting with the lower lumbar level (L6) using a Dumont #3 forceps (World Precision Instruments, #50037) and isolated by cutting connecting nerves with Vannas Spring Scissors (Fine Science Tools, #15000-00).

Halawani D., Wang Y., Ramakrishnan A., Estill M., He X., Shen L., Friedel R.H, & Zou H. (2023). Circadian clock regulator Bmal1 gates axon regeneration via Tet3 epigenetics in mouse sensory neurons. Nature Communications, 14, 5165.

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Margin Folding and Ablation Experiments

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Directional folding and ablation experiments shown in Figure 3: animals were pinned to sylgard plates, as described above for mouth pointing experiments. ~5ul of 0.2μm filtered shrimp extract was then pipetted directly onto either the top, bottom, left, or right portion of the margin. The timing of margin folding events from all quadrants, and the locations of sensory stimulation, were then manually annotated and compared. For physical ablation experiments, body parts were cut off using spring scissors (Fine Science Tools) or, to remove the mouth, by creating hole-punches using a blunt-tipped needle.

Weissbourd B., Momose T., Nair A., Kennedy A., Hunt B, & Anderson D.J. (2021). A genetically tractable jellyfish model for systems and evolutionary neuroscience. Cell, 184(24), 5854-5868.e20.

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Diaphragm Excision and Immunostaining

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Animals were euthanized by an intraperitoneal injection of ketamine/xylazine diluted in sterile saline and then placed in a supine position. A laparotomy was performed to expose the inferior surface of the diaphragm. The diaphragm was then excised using spring scissors (Fine Science Tools, Foster City, California), stretched flat and pinned down on silicon-coated 10 cm dishes, and washed with PBS (Gibco, Pittsburgh, Pennsylvania). Diaphragms were then fixed for 20 min in 4% paraformaldehyde (Electron Microscopy Sciences, Hatfield, Pennsylvania). After washing in PBS, superficial fascia was carefully removed from the surface of the diaphragm with Dumont #5 Forceps (Fine Science Tools, Foster City, California). Diaphragms were then stained for NMJ markers (described below).

Urban M.W., Charsar B.A., Heinsinger N.M., Markandaiah S.S., Sprimont L., Zhou W., Brown E.V., Henderson N.T., Thomas S.J., Ghosh B., Cain R.E., Trotti D., Pasinelli P., Wright M.C., Dalva M.B, & Lepore A.C. (2024). EphrinB2 knockdown in cervical spinal cord preserves diaphragm innervation in a mutant SOD1 mouse model of ALS. eLife, 12, RP89298.

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Diaphragm Muscle Preparation for NMJ Staining

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Animals were euthanized with a mixture of ketamine/xylazine/acepromazine. Animals were placed supine; two incisions were made into the skin and underlying muscle starting from the xyphoid process and extending laterally along the rib cage to expose the right hemi-diaphragm. The right hemi-diaphragm was excised using spring scissors (Fine Science Tools, Foster City, California), stretched flat and pinned down on silicon-coated 10 cm dishes, and washed with PBS (Gibco, Pittsburgh, Pennsylvania). Next, a 20-minute fixation in 4% paraformaldehyde (Electron Microscopy Sciences, Hatfield, Pennsylvania) was performed, followed by several washes in PBS. After washing, superficial fascia was carefully removed from the surface of the diaphragm with Dumont #5 Forceps (Fine Science Tools, Foster City, California). Diaphragms were then stained for NMJ markers (described below).

Urban M.W., Ghosh B., Strojny L.R., Block C.G., Blazejewski S.M., Wright M.C., Smith G.M, & Lepore A.C. (2018). Cell-type specific expression of constitutively-active Rheb promotes regeneration of bulbospinal respiratory axons following cervical SCI. Experimental neurology, 303, 108-119.

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Preparation of Retinal and Spinal Samples

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The animals were anesthetized with tricaine methanesulfonate (MS‐222, 200 mg/ml; Sigma) and transferred into an oxygenated Ringer's solution (in mM 130 NaCl, 2.1 KCl, 2.6 CaCl₂, 1.8 MgCl₂, 4 HEPES, 5 glucose, and 1 NaHCO₃, pH = 7.4) at room temperature. The skin and muscles were removed around the cranium with a fine forceps and spring scissors (Fine Science Tools). To provide access to the retina, the cornea, iris, and lens were removed. To provide access to the first five spinal segments, a dorsal laminectomy was performed. The preparations were then prepared for either anatomy or physiology experiments.

Flaive A, & Ryczko D. (2022). From retina to motoneurons: A substrate for visuomotor transformation in salamanders. The Journal of Comparative Neurology, 530(14), 2518-2536.

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Retinal Dissection and JAK2 Inhibitor Treatment

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P347S and P347S/miR‐181a/b‐1^+/− animals were sacrificed by cervical dislocation, following the institution's guidelines, at p30. Eyes were removed quickly using Dumont's forceps #5 and put in CO2‐independent medium—Gibco (18045‐054). Under a dissection microscope, the eyeball was opened and cut along the line between the anterior and posterior chambers of the eye using Spring scissors (Fine Science Tools). Lens were removed and the retina and RPE, attached in the inferior part of the eyeball, was dissected out using #5 forceps and flat‐mounted retina/RPE was placed in a new dish containing Dulbecco's modified eagle medium supplemented with 10% FBS (Euroclone) and 1% penicillin/streptomycin. The ex vivo retinas were treated with the JAK2 inhibitor FEDRATINIB (SAR302503, TG101348; Selleckchem) 100 μM for 8 h. Control retinas were treated with DMSO.

Carrella S., Di Guida M., Brillante S., Piccolo D., Ciampi L., Guadagnino I., Garcia Piqueras J., Pizzo M., Marrocco E., Molinari M., Petrogiannakis G., Barbato S., Ezhova Y., Auricchio A., Franco B., De Leonibus E., Surace E.M., Indrieri A, & Banfi S. (2022). miR‐181a/b downregulation: a mutation‐independent therapeutic approach for inherited retinal diseases. EMBO Molecular Medicine, 14(11), e15941.

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Zebrafish Caudal Fin Amputation

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Adult caudal fins were amputated by first anesthetizing the zebrafish with 0.2 mg/mL tricaine in fish-system water for approximately 5 minutes. The fish were next placed onto a clean paper towel, and their tails were snipped using spring scissors (Fine Science Tools, Cat. No. 91501-09). The fish were then allowed to recover in system water.

Mich J.K., Payumo A.Y., Rack P.G, & Chen J.K. (2014). In Vivo Imaging of Hedgehog Pathway Activation with a Nuclear Fluorescent Reporter. PLoS ONE, 9(7), e103661.

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