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Em ccd digital camera

Manufactured by Hamamatsu Photonics
Sourced in United States

The EM-CCD digital camera is a highly sensitive imaging device designed for low-light applications. It utilizes an electron-multiplying charge-coupled device (EM-CCD) sensor to amplify the signal, enabling the detection of extremely faint signals. The core function of the EM-CCD digital camera is to capture and digitize images with exceptional sensitivity, providing a powerful tool for scientific research and imaging applications where low-light conditions are a challenge.

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15 protocols using em ccd digital camera

1

Visualizing Amino Acid Starvation Responses

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Cells were grown at 32°C in EMM + aa to log phase (OD600 = 1). To visualize protein localization after amino acid starvation, cells were washed twice and resuspended in pre-warmed EMM –aa media for 90 min. Green fluorescent protein (GFP) tag was used to visualize GFP-tagged Bhd1 and Fnp1 proteins (FITC filter, 100-1000msec). FM4-64 dye was used to stain the vacuole membrane (RFP filter, 10-100msec) as described previously (Valbuena et al., 2012a (link)). Cell images were captured using an Olympus IX81 fluorescence microscope, equipped with Hamamatsu EM-CCD digital camera and processed using Slidebook software. FIJI program was used to measure the intensity of fluorescence. 2D Parallel Iterative Deconvolution plugin for Fiji program was used to perform the deconvolution of the fluorescence images.
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2

Live Imaging of Whole Worm Germline

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Whole worms were prepared for live imaging by anesthetic treatment with 0.5 mg/mL tetramisole-HCl in M9, and were then mounted on a 4% agarose pad and secured with a cover slip. Imaging was performed on a Leica DMI 4000B inverted compound microscope equipped with a Leica 63X/1.40–0.60 HCX Plan Apo oil objective lens. Image capture was accomplished using a Hamamatsu EM-CCD digital camera. Volocity (PerkinElmer Inc.) software was used to control the system. The entire germline was imaged by acquiring multiple stacks along the length of the gonad; each stack consists of 49 z-planes with a spacing of 0.5 μm. Visualization and analysis of the stacks were performed using ImageJ (http://imagej.nih.gov/ij/). Composite images were prepared using images from each stack corresponding to the same focal plane, and they were then stitched together using Adobe Illustrator.
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3

Fluorescence Imaging of Zinc Signaling

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Imaging experiments were performed using a Zeiss Axiovert 200M inverted epifluorescence microscope equipped with an EM-CCD digital camera (Hamamatsu) and a MS200 XY Piezo Z stage (Applied Scientific Instruments). The light source was an X-Cite 120 metal-halide lamp (EXFO) and the fluorescence images were obtained using an oil-immersion objective at 63× magnification. The fluorescence filters sets used are defined as blue: excitation G 365 nm, beamsplitter FT 395 nm, emission BP 445/50 nm; red: BP 550/25 nm, beamsplitter FT 570 nm, emission BP 605/70 nm. The microscope was operated using Volocity software (Perkin-Elmer).
The exposure time for acquisition of fluorescence images were kept constant for each series of images at each channel. To measure analyte-induced fluorescence changes, the cells were treated with dye-free DMEM containing 20 μM ZnCl2 and 50 μM pyrithione for 10 min. To reverse the effect of zinc, the cells were exposed to dye-free DMEM containing 50 μM TPEN for 15 min. All these experiments were carried out on the stage of the microscope. Quantification of fluorescence intensity was performed using ImageJ (version 1.45, NIH). The whole cell was selected as the region of interest. The integrated fluorescence from the background region was subtracted from the cell body region.
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4

Automated 3D Microscopy Imaging Protocol

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Data from immunohistochemistry experiments were collected on an Olympus (Center Valley, PA, USA) IX81 inverted microscope equipped with an Olympus spinning disk confocal unit, Hamamatsu EM-CCD digital camera (Bridgewater, NJ, USA), and high precision BioPrecision2 XYZ motorized stage with linear XYZ encoders (Ludl Electronic Products Ltd., Hawthorne, NJ, USA) using a 60× 1.40 N.A. SC oil immersion objective. The equipment was controlled by SlideBook 6.0 (Intelligent Imaging Innovations, Inc., Denver, CO, USA), which was the same software used for post-image processing. 3D image stacks (2D images successively captured at intervals separated by 0.25 μm in the z-dimension) that were 512 × 512 pixels (~137 × 137 μm; pixel size = 0.267 μm) were acquired over 50 percent of the total thickness of the tissue section starting at the coverslip. Importantly, imaging the same percentage, rather than the same number of microns, of the tissue section thickness controls for the potential confound of storage and/or mounting related volume differences (i.e., z-axis shrinkage). The stacks were collected using optimal exposure settings (i.e., those that yielded the greatest dynamic range with no saturated pixels), with differences in exposures normalized during image processing.
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5

Confocal Imaging of Muscle Samples

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A Leica TCS SP2 AOBS confocal microscope with Leica software, using an HC Plan Apochromat 20x/0.70 IMM CORR CS lens was used to image most muscle sections. A Zeiss 510 confocal microscope with Zen software, using a Plan-Apochromat 63x/1.40 lens, was used to image SB203580-treated and control transplant sections. Micrographs of local transplantation assays were captured with a Nikon Eclipse E800 equipped with a Sensicam (Cooke) digital camera and Slidebook v4.1 (3i) software with a PlanFluor 20x/NA 0.50 PH1 DLL (Nikon) lens. All other myofiber experiments were imaged with a Leica DM RXA Spinning Disk confocal microscope with EM-CCD digital camera (Hamamatsu) with Metamorph software (Molecular Devices), using HC Plan APO 20x/0.70 or HCX PL APO 40x/0.85 CORR lenses. All digital microscopic images were acquired at room temperature. The mounting medium for cells and sections was Vectashield Mounting Medium (Vector). Images were processed then scored with blinding in ImageJ64. As necessary, the brightness and contrast were adjusted linearly for the entire image and adjusted equivalently across the experimental image set. Muscle section images are averaged Z-stacks with Tikhonov-Miller deconvolution (ImageJ64) of the Syndecan-4, c-Met and Laminin channels.
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6

Confocal Imaging of Drosophila Brain

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Images were acquired with an Olympus IX81 inverted microscope equipped with a spinning disk confocal unit (Olympus), Hamamatsu EM‐CCD digital camera (Hamamatsu), and BioPrecision2 XYZ motorized stage with linear XYZ encoders (Ludl Electronic Products Ltd) using a 60× 1.4 NA SC oil immersion objective. 3D image stacks (2048 × 2048 pixels, 3 μm in 0.2 μm z‐steps) were taken to ensure full probe penetrance. Image sites were systematically and randomly selected across the fly brain using a grid of 100 μm2 frames spaced by 200 μm. Image collection was controlled by Slidebook 6.0 (Intelligent Imaging Innovations, Inc.). Differences in exposures were normalized during image processing.
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7

Fluorescent Dye Colocalization in A2780 Cells

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A2780 cells were seeded in an imaging dish in 2 mL of growth medium at 60% confluence. The growth medium was swapped with premixed medium containing 1–10 μM of TAMRA-mtDFO, and the cells were allowed to incubate with the dye for 1 h. MitoTracker Deep Red was added to the cells at 1.0–4.0 μM concentrations and allowed to incubate for 30 min. At the end of the incubation period, the medium was aspirated, and the cells were washed with 3 × 1 mL PBS and incubated with 2 mL of dye-free DMEM. The imaging experiments were performed using a Zeiss Axiovert 200M inverted epifluorescence microscope equipped with an EM-CCD digital camera (Hamamatsu) and a MS200 XY Piezo Z stage (Applied Scientific Instruments). The light source was an X-Cite 120 metal-halide lamp (EXFO), and the fluorescence images were obtained with an oil-immersion objective at 63× magnification. The microscope was operated by the Volocity software program of Perkin-Elmer. Colocalization of the dyes was quantitated using the program ImageJ using a previously described protocols [18 (link), 23 (link)].
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8

High-resolution Cortical Interneuron Imaging

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Images were acquired on an Olympus (Center Valley, PA, USA) IX81 inverted microscope equipped with an Olympus spinning disk confocal unit, a Hamamatsu EM-CCD digital camera (Bridgewater, NJ, USA), and a high-precision BioPrecision2 XYZ motorized stage with linear XYZ encoders (Ludl Electronic Products Ltd, Hawthorne, NJ, USA) using a 60x 1.40 NA SC oil immersion objective. Ten image stacks (512×512 pixels; 0.25 µm z-step) in layer 2 or 4 from each section were selected using a previously published method for systematic random sampling(24 (link)). Layer 2 or 4 was defined as 10-20% or 50-60% of the pia-to-white matter distance, respectively(25 (link)). We sampled these two layers as layer 4 contains a high density of PV interneurons(20 (link)) and prominently lower PV mRNA levels in schizophrenia(15 (link), 21 (link)), whereas layer 2 contains a high density of CR interneurons(26 (link)). The very low densities of PV interneurons in layer 2 and of CR interneurons in layer 4 precluded the sampling of these neurons. Lipofuscin for each stack was imaged using a custom fifth channel (excitation wavelength: 405nm; emission wavelength: 647nm) at a constant exposure time as previously described(27 ).
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9

Spinning Disk Confocal Imaging of 3D Tissue

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Data were collected on an Olympus (Center Valley, PA) IX81 inverted microscope equipped with an Olympus spinning disk confocal unit, Hamamatsu EM-CCD digital camera (Bridgewater, NJ), and high precision BioPrecision2 XYZ motorized stage with linear XYZ encoders (Ludl Electronic Products Ltd., Hawthorne NJ) using a 60× 1.40 N.A. SC oil immersion objective. The equipment was controlled by SlideBook 5.0 (Intelligent Imaging Innovations, Inc., Denver, CO), which was the same software used for post-image processing. 3D image stacks (2D images successively captured at intervals separated by 0.25 µm in the z-dimension) that were 512 × 512 pixels (~ 137 × 137 µm) were acquired over 50 percent of the total thickness of the tissue section starting at the coverslip. Importantly, imaging the same percentage, rather than the same number of microns, of the tissue section thickness controls for the potential confound of storage and/or mounting related volume differences (i.e. z-axis shrinkage). The stacks were collected using optimal exposure settings (i.e., those that yielded the greatest dynamic range with no saturated pixels), with differences in exposures normalized during image processing.
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10

Confocal Imaging of Muscle Samples

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A Leica TCS SP2 AOBS confocal microscope with Leica software, using an HC Plan Apochromat 20x/0.70 IMM CORR CS lens was used to image most muscle sections. A Zeiss 510 confocal microscope with Zen software, using a Plan-Apochromat 63x/1.40 lens, was used to image SB203580-treated and control transplant sections. Micrographs of local transplantation assays were captured with a Nikon Eclipse E800 equipped with a Sensicam (Cooke) digital camera and Slidebook v4.1 (3i) software with a PlanFluor 20x/NA 0.50 PH1 DLL (Nikon) lens. All other myofiber experiments were imaged with a Leica DM RXA Spinning Disk confocal microscope with EM-CCD digital camera (Hamamatsu) with Metamorph software (Molecular Devices), using HC Plan APO 20x/0.70 or HCX PL APO 40x/0.85 CORR lenses. All digital microscopic images were acquired at room temperature. The mounting medium for cells and sections was Vectashield Mounting Medium (Vector). Images were processed then scored with blinding in ImageJ64. As necessary, the brightness and contrast were adjusted linearly for the entire image and adjusted equivalently across the experimental image set. Muscle section images are averaged Z-stacks with Tikhonov-Miller deconvolution (ImageJ64) of the Syndecan-4, c-Met and Laminin channels.
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