Assignment 3, Part 1: visualizing actin with fluorescence contrast

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20.309: Biological Instrumentation and Measurement

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This is Part 1 of Assignment 3.

3T3 Actin.png

3T3 Actin plus CytoD.png

3T3 cells. Actin stained with Alexa Fluor 568 Phalloidin.

Same cell type incubated with cytochalasin D, an inhibitor of actin polymerization, prior to fixing and stained.

Fluorescent staining

In this part of the lab, you will use fluorescence microscopy to investigate the effect of a toxin called cytochalasin D on cultured epithelial cells. Cytochalasin D inhibits the of polymerization of [actin]. Actin is an important component of the cytoskeleton. Exposure to cytochalasin D causes marked changes in the shape and mechanical properties of cells. In this part of the lab, you will make and compare images of healthy (control) cells and identical cells that have been exposed to cytochalasin D. We will investigate some of the mechanical changes in the next part of the lab.

The actin structures we wish to examine is are normally visible under a microscope. There are (at least) three feasible approaches to creating contrast — all involving fluorescence:

  1. use genetic manipulations to modify the actin protein so that it fluoresces,
  2. use an antibody conjugated to a fluorescent dye, or
  3. use a (non-antibody) compound conjugated to a fluorescent dye.

Each of the approaches has advantages and drawbacks. We will use the third approach. The mushroom toxin phalloidin binds to polymerized filamentous actin (F-actin) much more tightly than to actin monomers (G-actin), and stabilizes actin filaments by preventing their depolymerization. You will take advantage of this strong affinity between phalloidin and F-actin to image the cell's actin cytoskeleton. Phalloidin conjugated with the fluorescent dye Alexa Fluor 568 will be introduced in 3T3 mouse fibroblast cells.

By comparing Alexa Fluor phalloidin-stained untreated cells and CytoD-treated cells, you will observe and quantify the effect CytoD has on the actin stress fiber network. Cytochalasin D is also a mycotoxin, but contrary to phalloidin, it poisons the cell by strongly inhibiting actin polymerization.

20.309 130904 PhalloidinActin.png Alexa568.jpg
Example of a NIH 3T3 fibroblast cell labeled with rhodamine phalloidin Excitation and emission spectra for Alexa Fluor 568


Warning.jpg Wear gloves and lab coats when you are handling biological samples.


Procedures for fixing and labeling cells

3T3 Swiss Albino

You will be given two plates of cells:

  • one dish will be left untreated, and then fixed and labeled with phalloidin;
  • the second dish will be first treated with CytoD, and then fixed and labeled with phalloidin.

A key technique to keep in mind when working with live cells - to avoid shocking them with "cold" at 20°C - is to be sure that any solutions you add are pre-warmed to 37°C. We will keep a warm-water bath running for this purpose, in which we will keep the various media.

You are provided with 3T3 cells, which were prepared as follows: Cells were cultured at 37°C in 5% CO$ _2 $ in standard T75 flasks in a medium referred to as DMEM++. This consists of Dulbecco's Modified Eagle Medium (DMEM - Invitrogen) supplemented with 10% fetal bovine serum (FBS - Invitrogen), 1% of the antibiotic penicillin-streptomycin (Invitrogen), 1% non-essential amino acids, and 1% glutamine. The day prior to the fluorescence imaging, cells were plated on 35 mm glass-bottom cell culture dishes (MatTek, equipped with coverslip suited for optical microscopy studies).

Please read through the protocol for the two dishes below. Think about what you need to do so you can handle the dishes in parallel and save yourself some time.

Below is the protocol to stain 3T3 cells with Alexa Fluor 568 phalloidin:

  • It is optimal for your cells to be ~60% confluent. If cells are too crowded, they will not stretch properly and show their beautiful actin filaments. Thus, you'll want to image cells that are stretched out and not overlapping much. Note also that these cells remain alive until the addition of formaldehyde, therefore requiring that any buffer/media added be pre-warmed.
  1. Pre-warm 3.7% formaldehyde solution and phosphate buffered saline at pH 7.4 (PBS) in a 37°C water bath if available. Keep the formaldehyde wrapped in foil to protect from light.
  2. Retrieve an aliquot of cytochalasin D from the freezer and warm to 37°C.

Dish 1--CytoD Treated Cells

  • Prepare only ONE dish to be treated with cytochalasin D (CytoD). The other dish will be an untreated control.
  1. Remove the medium with a pipette and wash ONE dish 2X with 2 mL of pre-warmed PBS. Pipet into the dish gently to avoid washing away cells.
  2. Add 1 mL of the pre-warmed 10 μM CytoD solution to the same cell culture dish and incubate at 37°C for 15 minutes (and not a minute longer!). Afterwards, wash 2X with PBS.

Dish 1 (CytoD) & Dish 2 (Untreated) Stained in Parallel

  1. Remove the medium from the untreated dish (Dish 2) with a pipette and wash 2X with 2 mL of pre-warmed PBS. Pipet gently to avoid washing away cells. This assumes you've already washed your Cyto D plate (Dish 1).
  2. Carefully pipet 400 μL of 3.7% formaldehyde solution onto the cells in the central glass region of each dish and incubate for 10 minutes at room temperature. This "fixes" the cells, i.e. cross-links the intracellular proteins and freezes the cell structure.
  3. Wash each dish 3X with 1.5 mL PBS (note that this PBS solution no longer needs to be pre-warmed as the cells are dead).
  4. Extract each dish with 1.5 mL 0.1% Triton X-100 (a detergent) for 3-5 minutes. (Extraction refers to the partially dissolution of the plasma membrane of the cell.)
  5. Wash the cells 2X with 1.5 mL PBS.
  6. Incubate the fixed cells with 1.5 mL 1% BSA in PBS for 20 minutes. (BSA blocks the nonspecific binding sites.)
  7. Wash each dish 2X with PBS.
  8. Add 200 μL of Alexa Fluor 568 phalloidin solution (pre-mixed in methanol and PBS) to each dish. Carefully pipet this just onto the center of the dish, cover with aluminum foil, and incubate for 45 minutes at room temperature.
  9. Wash 3X with PBS, leaving the last wash of PBS in the dish so the cells don't dry out.
  10. Imaging your samples right away will give you the best results. However, the samples can be stored at +4°C (regular refrigerator) in PBS for a few days, wrapped in parafilm and foil.

Fluorescence imaging

In this part of the lab, you will make images of fluorescent microspheres plus your dishes of cells, and correct them for nonuniform illumination. In order to do the correction, you will need a reference image and dark images in addition to the image of the sample. See this page for more information about flat-field correction.

  • Reference Images: Take the reference image as close as possible in time to the sample images. Don't make any adjustments to your microscope between capturing the reference image and the sample image. For example, every time you move a mirror or re-align the laser, you will change the illumination profile and you must take a new reference. Adjusting the camera exposure and gain between recording the reference and sample images is okay.
  • Dark images: Each time you record an image (reference or sample), make sure to take a corresponding dark image using the EXACT SAME camera settings (i.e. use the exact same Exposure Time and Gain settings you had chosen for your reference/sample image). This is the only valid way to subtract the correct dark value from your reference/sample image. Use 12-bit imaging mode to get the best results.
  • Saving: Remember to save your images in a format that preserves all 12 bits. We recommend using the MATLAB save command to save data in a .mat file so you can reanalyze it later if necessary. You could also save in an image file format with imwrite. Convert the image to 16-bit, unsigned integer format with the correct range before saving. Go back and read this page if you need to refresh your memory.

Tips

A few tips to keep in mind as you go:

  • Visualizing the actin cytoskeleton under your 20.309 microscope will require mad skills. Since actin filaments and stress fibers are nanometer-scale objects, they are much dimmer than fluorescent beads or the dye solution - care must be taken to get good images of the cytoskeleton.
    • You may need to cover the microscope or turn off the overhead lights to reduce room light contamination.
    • As soon as you expose the sample to laser light, the fluorescent dye will start to photobleach. You may find it helpful to use your brightfield microscope to find your cells before turning on your laser illumination.
    • Once you've found cells in the brightfield, turn off the LED and turn on the laser. Fine tune the focus using a high gain/low exposure setting. (This setting will give you poor images with a lot of noise, but it's hard to focus the sample with a long exposure time.)
    • Finally, adjust the gain (to zero) and increase the exposure of the camera to get the best picture.
  • For each microscopy sample, remember to check the exposure time, and take a corresponding dark image. Have someone record the camera settings used for each image.

Take images

  1. Record a reference image
    • Put in an ND filter and take an image of the reference slide with the 40X objective.
    • Use the histogram in the UsefulImageAcquisitionTool to be certain that the image is exposed correctly
    • Turn off the laser and record a dark image (without changing any camera settings!)
  2. Remove the ND filter and image the samples:
    • Fixed and stained untreated cells and a corresponding dark image
    • Fixed and stained cells treated with CytoD and a corresponding dark image
    • Again, be certain that the images are exposed correctly



Example image of CHO cells whose actin network is labeled with Alexa Fluor phalloidin

Flat field correction

Perform flat-field correction on the images.

  • Divide the image by a normalized version of your reference image minus the dark image (see this page for more detail).


Pencil.png Turn in a figure with images of the the stained cell samples with and without Cyto-D.
    • For each sample, create 1 figure with 5 panels.
    • The panels of the figure should be: A) unprocessed image; B) reference image; C) dark image; D) flat-field corrected image; and E) histogram.
    • In the caption, specify the exposure and gain settings. Each image should have a scale bar (you may find this page handy). State the dimension of the scale bar in the caption.
    • For panel E, plot histograms of the unprocessed, dark, reference, and corrected image on the same set of axes. Plot log10( count ) on the vertical axis and intensity on the horizontal axis. Use a line plot instead of a bar chart for the histogram.
  1. Image profile
    • For one reference, dark and cell image set, plot an intensity profile across the same diagonal. You may also use a bead image, along with it's unique reference and dark images. The intensity of your three images should be on the same scale, i.e., 0 to 65,535 or 0 to 1. Place all three profiles on a single set of axes for comparison. (Use the improfile command in MATLAB.)
  2. Discussion
    • How did your beam expander design affect your images?
    • What differences did you observe between the cells with and without CytoD?


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