Information

Is there any reason to use an upright microscope over an inverted microscope?

Is there any reason to use an upright microscope over an inverted microscope?


We are searching data for your request:

Forums and discussions:
Manuals and reference books:
Data from registers:
Wait the end of the search in all databases.
Upon completion, a link will appear to access the found materials.

I've never actually owned an inverted microscope, but it seems it has only advantages compared to an upright microscope: taller, heavier samples; no crashing the objective into the glass slide; easier to operate, etc.

Why then do people still use regular, upright microscopes? Is there a disadvantage I'm missing?


As already mentioned in the comments, cost is one of the primary reasons when you're looking at simple light microscopes. Inverted scopes have more complex optics, along with the convenience factor of being able to examine larger samples, generally having a more stable frame, etc. All this leads to higher cost.

An advantage I can think of for smaller upright scopes is the ability to use them as a dissecting scope, where the sample is opaque and you need to see it from above. Another advantage is this:

Many fluorescence microscopes are upright, as there is a significant amount of extra equipment that needs to be mounted in addition to the eyepiece, including lasers, stage motors, and cameras and other detectors. This can take up a lot of room, and for convenience's sake it's often easiest to mount it up top where it is accessible.


What Is An Inverted Microscope?

Microscopes are used in many scientific processes, especially when it comes to observing small objects, including cells.

Whether it’s for traditional medical science or forensics, microscopes are essential instruments. However, as science progresses, new technological advances are designed to provide greater magnification to achieve better results. This is where an inverted microscope enters the picture.

But, if you’re new to this innovation in the field of science, keep reading this article to learn more about the inverted microscope.


INTRODUCTION

Most broadly, light microscopy techniques can be divided into two categories: brightfield and fluorescence. In brightfield microscopy, the light source and detection objective are placed on opposite sides of the sample, and the sample is imaged by its effect on the light passing through it as the sample absorbs, scatters, or deflects the light. Because most cells are thin and transparent, they do not absorb much light and so are difficult to see without adding optics that allows the phase shift of light induced by the cells to be seen. The two most commonly used techniques to visualize this phase shift are phase contrast, which causes cells to appear dark on a light background, and differential interference contrast (DIC), which gives a pseudo–three-dimensional (3D) shaded appearance to cells (Murphy and Davidson, 2012). Brightfield without phase contrast or DIC is usually sufficient to see the general outlines of cells, but phase contrast or DIC is necessary to achieve detailed, high-contrast brightfield images.


Different Microscopes

The simplest form of a microscope is a magnifying glass. You may not really think of it as a microscope, but it is! It magnifies an image, but it does not invert the image or magnify it enough to truly see tiny things like cell structures or other details that are necessary for microscopic scientific studies.

What you would normally classify as a microscope is what you see in a school classroom or on a scientific TV show, and these are called compound microscopes. Compound microscopes invert images! They do this because of the two lenses they have and because of their increased level of magnification. That is also what makes them recognizable.

Obviously, other kinds of microscopes also flip images over, and there are others with an additional lens that re-inverts the image back to its original orientation. This means that the image you see has been inverted and then inverted again to be the same position it was in originally.

Quite a few microscopes, including electron microscopes and digital microscopes, will not show you inverted images. Binocular and dissecting microscopes will also not show an inverted image because of their increased level of magnification. Where you are at and what kind of work you are doing has a lot to do with what kind of image you are looking at.

Even with an inverted image, microscopes can increase the magnification of an image phenomenally. They have helped the world to progress by helping doctors, engineers, students, and everyone else to see a world beyond the one we see with our naked eye. They have brought about amazing feats in the medical field with tissues and cells as well as diseases and antibiotics.

Not only does it help us progress in the structures we create and the procedures we perform, but it also helps in fields like forensic science, biology, and the study of germs, viruses, and bacteria. Microscopic images help us to see the world from a new perspective that would be impossible without them. We just need to recognize when the image is right-side up!

Brandon is an enthusiast, hobbyist, and amateur in the world of microscopy. His love for science and all things microscopic moves him to share everything he knows about microscopy and microbiology.

Recent Posts

Learning to see the world from a minuscule point of view creates an immense difference in our perspective of life. Whether you are a teacher, student, or just a microscope enthusiast, these riveting.

By understanding the microorganisms that live beyond what the human eye can see, we can better understand our history as living beings. Amongst this microscopic world of organisms are.


Olympus FV3000: Basic Microscope Operation

Important note- the FV3000 is an inverted microscope, which means people will use a wide variety of containers for their specimens. There is also the option of using the stage top incubator, which puts specimens up even higher. What this means is that the focal plane can and will be all over the place, and you should be prepared to take some time to find it for your specimen.

I. Controlling XYZ movement

These controls are on the right side of the air table. Turning the focus knobs towards you raises the objectives (towards the specimen) turning them away from you lowers the objectives. When using oil objectives with short working distances, you should be primarily using the fine focus knob. The X-Y knobs should be exclusively used to move the stage.

This device controls the view mode (eye pieces or confocal), the form of illumination for the eye pieces (Epi-fluorescence or DIC bright field), the objectives, and allows you to record 8 separate x-y coordinates so that you may send the stage to regions of interest.

The “Escape” button lowers the objective turret, which is needed for the use of oil objectives (covered in detail later).

The “Focus Search” function is a nice shortcut that finds the coverslip. If the device successfully fines the coverslip, you will hear one beep (good). If it can’t you will hear 3 beeps (bad). If it fails, the most likely cause is a previous user who used a very different specimen container and shifted the focal plane. Your best bet is to go to the 2x objective to focus on the edge of a coverslip or well, then switch back to the 10x to find your target. You can then reset the Z origin and the Z-limit (if needed) in the Fluoview software. The search function will also fail if the ZDC DM is “Out” instead of “In” (“Microscope” Tab in the Fluoview software).

The “EPI” tab allows you to control the filter cube:

There are 3 filters available: DAPI, FITC (green/yellow fluors), and TRITC (orange/red fluors). There are no filters for viewing dyes that fluoresce in the 600+ nm range, but you will be able to see them in confocal mode with the 640 nm laser.

The “DIA” screen option is most commonly used to adjust the light intensity.

You have a choice of 3 stage inserts for your fixed specimens: 1) the well plate holder, 2) the universal slide holder (which you can use for a single slide or a 60mm or smaller dish), and 3) the 4-slide holder. Remember to place your slide coverslip down. If you use a plastic vessel, you are limited to the air objectives (2x, 10x, and 20x). If you want to use an oil objective, you must use a glass bottom or cover slip of the proper thickness (

IV. The Tokai Hit stage enclosure

Our system includes a stage enclosure because our room is drafty and we cannot control the thermostat. For fixed specimens you can leave the front hatch up. For a time-lapse scan of any great length, you have the option to put this lid down to keep the stage environment more stable. This enclosure does introduce an extra step in tilting back the condenser (which you need to do when placing stage inserts or oiling/ wiping off objectives).

To open the space around the condenser, push the two sliders (red arrows) outwards. You can then push up and back on the condenser focus knobs to tilt it back. You can leave the top open in you don’t need to keep drafts off the stage. The one downside of this arrangement is that it is very easy to forget to tilt the condenser back. If you don’t get an image in confocal mode, the first thing you should do is glance left to check if you see this. The lasers will be blocked unless the condenser is down.

V. Switching from Air to Oil Objectives

An inverted microscope allows you to image specimens in well plates or dishes or well slides with higher N/A oil objectives by putting those objectives underneath, so that oil does not contaminate the specimen. The downside is that oiling the objectives is trickier than it is for an upright system. The oil drop in an inverted configuration will be perched a bit precariously on the tip of the objective lens, and it needs to stay between the lens and the coverslip/ dish bottom. Too little oil, and you won’t have a proper path for the light. Too much oil, and it will start to run down the sides of the objective once it makes contact with the other piece of glass. Getting that usable blob of oil between the pieces of glass is an art form, and even experienced users may have to try several times. Once you get it placed properly, you can move the stage around within the limits of your oil blob and take multiple images. But when you have to image beyond the range of your current oil blob, or you’re changing specimens, you will need to wipe all the oil off the objective with the lens paper, and apply a new drop. It’s a hassle, but necessary, because too much oil flows down, which is bad for multiple reasons.

If you are using a well plate, you will need to pre-oil the oil objective you plan to use before you put your plate into the stage.

We have 2 types of oil: the blue bottle (ne = 1.518) for the 60x objective, and the green bottle Silicone oil (ne = 1.406) for the 30x and 40x Si objectives.

A few more details on Objective switching

There is a button at the bottom left of the stage enclosure that will switch on a light to illuminate that space, which makes it easier to see for oiling objectives. Remember to switch it back off before you start imaging. The knob next to it controls the brightness.

The universal stage insert is the easiest to use when oiling objectives, as there is open space all around your specimen holder to use for access to the objective. With the 4-slide insert there is enough open space on the left or right side to use, even if you mount 4 slides. If you are using a well plate or the stage top incubator, you will need to pre-oil your objective, then switch to the 2x or 10x before you put your specimen/ the chamber into the stage opening.

When an objective is “escaped”, do not touch any focus knobs. If you do, it will “un-escape” and move back up. The point of using this function is to prevent collisions between the objectives and the stage insert. The Fluoview software will be greyed-out and inactive while an objective is Escaped.

To remove oil from your slide, blot with lens paper (in the box on the computer desk), and then wipe the rest off with a bit of ethanol. DO NOT use Kimwipes on objectives or anything (like slide or dishes) that will be near objectives. Your specimen holders should be free of oil when you bring them into the Core, especially if you have previously viewed them with oil on a different brand of microscope. Each microscope manufacturer has their own version of immersion oils, with different refractive indices, so they are not compatible.


Upright Metallurgical Microscopes

What differentiates upright metallurgical microscopes from the others is that the illumination system is located above the sample stage, which allows light to be directed (from objectives) onto the sample and back to the eyepieces.

The microscope may come with a pillar stand or the typical base stand depending on the needs of the user. For instance whereas the typically base stand allows for more stability of the microscope to be used for relatively small samples, the pillar stand allows for enhanced flexibility allowing for different sized samples to be viewed.

Some of the features of the upright microscope include an adjustable intensity control, a diopter, 10x wide field eyepieces as well as plan achromatic infinity corrected objectives.

MicroscopeMaster Upright Metallurgical Reviews:

While the different types of metallurgical microscopes present an advantage depending on their intended use, the inverted microscope has been shown to have a number of advantages over the upright microscope. These include:

More freedom - With the inverted microscope, optics are located below the microscope stage while the sample is typically placed above the objectives. This eliminates the limitations that the upright microscope faces with regards to the size of the sample.

Here, the user benefits from the greater working distance, which allows for bigger and heavier samples to be placed on the microscope for observations (up to 30kg)

Efficiency - Using an inverted microscope, users benefit from the fact that they view more samples within a shorter period of time.

For an upright microscope, viewing the sample involves a number of steps including lowering the stage, adjusting it, taking care to protect the sample on the stage holder etc. This is not the case with the inverted microscope given that the user can simply place the object on the stage and image it after focusing.

Focus is retained for different magnifications, which means that for the same type of sample, the user would find viewing easier.

The objective is protected - The objective of the inverted microscope is located beneath the stage in addition to the presence of a focus stop functionality (with some microscopes) which protects the objective at all times minimizing chances of damage. This is not the case with upright microscopes where the objective is above the sample stage where it can come into contact with the sample or other hard objects at any given time.


Authors Biography & Contact Information

Bio: Robert Berdan is a professional nature photographer living in Calgary, AB specializing in nature, wildlife and science photography. Robert retired from CellNeurobiology research to take up photography full time years ago. Robert offers photo guiding and private instruction in all aspects of nature photography and Adobe Photoshop training - including photomicrography and macrophotography. Portrait of Robert Berdan with pictures from some of his science publications taken by Dr. Sharif Galal. His first research microscope is shown on the right.


Information

Others

Avantor ® , a Fortune 500 company, is a leading global provider of mission-critical products and services to customers in the biopharma, healthcare, education & government, and advanced technologies & applied materials industries. Our portfolio is used in virtually every stage of the most important research, development and production activities in the industries we serve. One of our greatest strengths comes from having a global infrastructure that is strategically located to support the needs of our customers. Our global footprint enables us to serve more than 225,000 customer locations and gives us extensive access to research laboratories and scientists in more than 180 countries. We set science in motion to create a better world. For information visit, www.avantorsciences.com and find us on LinkedIn, Twitter and Facebook.

© 2021 VWR International, LLC. All rights reserved.
© 2021 FORTUNE Media IP Limited All rights reserved. Used under license.


Is there any reason to use an upright microscope over an inverted microscope? - Biology

Stephen M. Wolniak
Professor
Department of Cell Biology & Molecular Genetics
University of Maryland
College Park, Maryland, 20742
[email protected]

Teaching Interests - Microscopy

I provide the information presented below for students who generally know little about the basics of image formation in the light microscope. If you wish to use this information, kindly credit (blame) me for the effort it took to generate the document.

Principles of Microscopy


Brightfield microscopy

The microscope that is available to you for general use in this laboratory is a sophisticated optical instrument that can provide you with high-resolution images of a variety of specimens. Image quality is based largely on your ability to use the microscope properly. Below you will find some basic information that you have probably heard before, but information that is rarely presented in a thorough way.

The magnification of small things is a necessary facet of biological research, but the fine detail in cells and in subcellular components requires that any imaging system be capable of providing spatial information across small distances. Resolution is defined as the ability to distinguish two very small and closely-spaced objects as separate entities. Resolution is best when the distance separating the two tiny objects is small. Resolution is determined by certain physical parameters that include the wavelength of light, and the light-gathering power of the objective and condenser lenses. A simple mathematical equation defines the smallest distance (dmin) separating the two very small objects:


dmin = 1.22 x wavelength / N.A. objective + N.A. condenser

This is the theoretical resolving power of a light microscope. In practice, specimen quality usually limits dmin to something greater than its theoretical lower limit.

N.A. (Numerical Aperture) is a mathematical calculation of the light-gathering capabilities of a lens. The N.A. of each objective lens is inscribed in the metal tube, and ranges from 0.25-1.4. The higher the N.A., the better the light-gathering properties of the lens, and the better the resolution. Higher N.A. values also mean shorter working distances (you have to get the lens closer to the object). N.A. values above 1.0 also indicate that the lens is used with some immersion fluid, such as immersion oil.

From the equation above, you should be aware that the N.A. of the condenser is as important as the N.A. of the objective lens in determining resolution. It is for this reason that closure of the condenser diaphragm results in a loss of resolution. In practice, at full aperture and with good oil immersion lenses (N.A. 1.4 for both the condenser and the objective) it is possible to be able to resolve slightly better than 0.2 µm. From the equation above, it should also be clear that shorter wavelength light (bluer light) will provide you with better resolution (smaller dmin values). However, there are practical considerations in how short the wavelength can be. In the early 1950's, a UV microscope was designed, but required quartz objectives and a specialized imaging device. The quartz lenses provided slightly better resolution (dmin = 0.1 µm), but image quality suffered from an inability on the part of the manufacturers to correct for aberrations caused by the quartz. The human eye is best adapted for green light and our ability to see detail may be compromised somewhat with the use of blue or violet. Most manufacturers of microscopes correct their simplest lenses (achromats) for green light.


- Magnification and Imaging -

Most microscopes in current use are known as compound microscopes, where a magnified image of an object is produced by the objective lens, and this image is magnified by a second lens system (the ocular or eyepiece) for viewing. Thus, final magnification of the microscope is dependent on the magnifying power of the objective times the magnifying power of the ocular. Objective magnification powers range from 4X to 100X. Lower magnification is impractical on a compound microscope stand because of spatial constraints with image correction and illumination. Higher magnification is impractical because of limitations in light gathering ability and shortness of working distances required for very strong lenses. Ocular magnification ranges are typically 8X-12X though 10X oculars are most common. As a result, a standard microscope will provide you with a final magnification range of

Each objective lens consists of six or more pieces of glass that combine to produce a clear image of an object. The six or more lenses in the objective lens are needed to provide corrections that produce image clarity. The interaction of light with the glass in a lens produce aberrations that result in a loss in image quality because light waves will be bent, or refracted, differently in different portions of a lens, and different colors of light will be refracted to different extents by the glass. Spatial aberrations (e.g., spherical aberration) can be corrected by using lenses with different curvature on their surfaces, and chromatic (i.e., color) aberrations can be minimized by using multiple kinds of glass in combination. These corrections increase the cost of the lens to the extent that an apochromatic objective lens exhibiting full color correction and extremely high N.A. can cost several thousand dollars. This objective lens is about the size of your thumb.

The objective lenses in most microscopes are achromats, and best suited for imaging with green light. Green filters narrow the bandwidth of the light, and make achromat objectives reasonably effective for most routine uses. The achromat lenses are not suitable for critical high-resolution imaging with white light, because red and blue light do not focus in the same plane as green light. Chromatic aberrations will degrade resolution in color images obtained with achromatic objectives. Color photomicrography aimed at the highest level of resolution and image clarity should be performed with totally corrected apochromatic objective lenses. Fluorite lenses, offer intermediate levels of correction, better than achromats but not as good as apochromats. Fluorite lenses are well suited for fluorescence microscopy because of their high transmittance of shorter wavelength light. Higher levels of correction make objective lenses more expensive the price range for apochromatic objectives goes from about $3,000 to over $10,000.

The oculars in most microscopes are designed to work optimally with the objective lenses from the same manufacturer. Each manufacturer makes some of the color and spatial corrections in the objective and the remainder of the corrections in the ocular. Mixing brands will usually result in a degraded image. In addition, when you look into a microscope, the magnified and corrected image you see through the oculars is actually a virtual image (as opposed to a real image). The ocular, designed to provide a corrected virtual image when viewed by eye, is not suitable for the generation of photographic or video images through the microscope. For photography or video microscopy it is necessary to use a projection lens that generates a corrected real image. Many of the newer microscopes provide total image corrections in the objective lens, thus obviating many of the concerns aboout matching glass components from the same manufacturer. Nevertheless, it is a good practice not to mix parts from one manufacturer with those of another, because unintended image degradation can result.

An essential factor in producing a good image with the light microscope is obtaining adequate levels of light in the specimen, or object plane. It is not only necessary to obtain bright light around the object, but for optimal imaging, the light should be uniform across the field of view. The best way to illuminate the specimen involves the use of yet another lens system, known as a condenser. The front element of the condenser is usually a large, flattened lens that sits directly beneath the specimen. Its placement on a movable rack provides you with the means to focus the light beam coming past the object and maximixe the intensity and control the uniformity of illumination. Two apertures in the illumination system allow you to regulate the diameter of the illumination beam by closing or opening iris diaphragms. One of these diaphragms, housed within the brightfield condenser and known as the condenser diaphragm, allows you to increase contrast, but at the cost of worsening resolution. The second of these diaphragms, known as the field aperture diaphragm, does not affect resolution as dramatically and is regularly adjusted for optimal illumination.

Optimal illumination of a specimen with all microscopes currently manufactured is achieved by using a variation of Kohler Illumination, where (for those of you are technophiles) the filament of the light source is in focus at the rear focal plane of the objective lens. Operationally, it is easy to obtain optimal illumination for brightfield (or phase contrast) by first placing any specimen on the stage and focusing on the object. Next, turn the ring for the field aperture diaphragm (the lowest aperture on the microscope) so that its edges obscure the periphery of the field of view. Next, raise or lower the condenser until the edges of the field aperture diaphragm are clearly focused. Do not refocus the objective on the specimen while you are adjusting the condenser. It may be necessary to center the field aperture diaphragm, using the condenser centering screws. When the microscope is properly illuminated, both the object and the edges of the field aperture diaphragm should be in the same plane of focus and the field iris diaphragm should be centered in the field of view.


Phase Contrast Microscopy

The human eye can perceive changes in light amplitude (intensity). Unstained biological specimens, such as living cells, are essentially transparent to our eyes, but they interact with light in a fairly uniform way, by retarding (slowing) the passage of a light beam by approximately 1/4 of a wavelength ( />). By slowing a light beam this much relative to another light beam that had passed though the surrounding medium, the biological specimen alters the phase of the beams. Intensity (amplitude) is additive and light rays that are 1/2 />out of phase are perceived as darkness. Zernicke realized that if he could retard the light passing through biological specimens without affecting the light passing through the surrounding medium, he could generate changes in amplitude within living cells. The phase contrast microscope was invented by Zernicke in the 1930's as a means to generate contrast in biological specimens, changing these invisible phase differences into visible amplitude differences.

Zernicke employed an optical trick to separate the light beams interacting with the specimen from those that do not encounter the specimen. To separate the beams of light from each other, he placed a transparent ring (known as an annulus) in an opaque disk and inserted this disk into the optical path of the microscope, within the condenser. He placed a complementary ring inside the objective lens. Nearly all of the light that passes through the sample but misses the specimen then passes through the objective lens through this ring. Most of the light that passes through the specimen is scattered and some of it enters the objective lens in such a way that it will not pass through the objective lens ring, but will pass this plane in some other location. He designed the glass plate holding the ring so that all light missing the ring would encounter an additional 1/4 />of retardation relative to the beams of light that had not interacted with the specimen, placing the light rays that had interacted with the specimen out of phase with rays that had not interacted with the specimen by 1/2 />. He found that a reduction in intensity of the light that had not passed through the specimen would create a grey background and increase contrast even more, with some parts of the specimen darker and other parts of the specimen brighter than the background.

The operation of any microscope in the phase contrast mode requires that you first set up proper brightfield illumination, with a centered field iris diaphragm whose edges are in focus in the specimen plane. Next, rotate the condenser turret cylinder until the number on the condenser turret matches the number engraved on the objective lens. Under this condition, the condenser annulus is matched to the phase ring present in the objective. Next, remove one of the oculars and insert the Bertrand focusing telescope into the ocular hole. This lens enables you to see the rear focal plane of the objective lens, the plane where the ring resides. You will see a bright circle of light (the condenser annulus) and a dark ring (present within the objective). The dark ring is stationary, but the bright annulus is not. You may need to align the annulus with the ring so that the two are superimposed. On the back side of your condenser, you will find two adjustment screws that permit this alignment to be performed. When the ring and the annulus are aligned, place the ocular back into the microscope. The difference between phase contrast and brightfield for the observation of living cells is significant.

Fluorescence Microscopy

In certain classes of atoms and molecules, electrons absorb light, become energized, and then rapidly lose this energy in the form of heat and light emission. If the electron keeps its spin, the electron is said to enter a singlet state, and the kind of light that is emitted as the electron returns to ground state is called fluorescence. If the electron changes its spin when excited, it enters the triplet state, and the kind of light that is emitted as the electron returns to ground state is known as phosphorescence. Phosphorescence is much longer-lived than fluorescence. Both fluorescence and phosphorescence emissions are of particular wavelengths for specific excited electrons. Both types of emission are dependent on specific wavelengths of excitation light, and for both types of emission, the energy of excitation is greater than the energy of emission. Described another way, />of excitation light is shorter than />of emission light. In biology, we can utilize fluorescence in localization reactions, to identify particular molecules in complex mixtures or in cells. Fluorescence has the advantage of providing a very high signal-to-noise ratio, which enables us to distinguish spatial distributions of rare molecules. To utilize fluorescence, we need to label the specimen (a cell, a tissue, or a gel) with a suitable molecule (a fluorochrome) whose distribution will become evident after illumination. The fluorescence microscope is ideally suited for the detection of particular fluorochromes in cells and tissues.

The fluorescence microscope that is in wide use today follows the basic "incident-light" design of Ploem, who employed a novel arrangement of filters with a chromatic beam splitter (often wrongly called a dichroic filter both by biologists and microscope sales people). With the incident light fluorescence microscope, the object is illuminated with fluorescence excitation light through the objective lens. The object emits longer-l fluorescence in response to the shorter- excitation light. The objective lens then serves both for illumination and imaging. The chromatic beam splitter transmits or reflects light, depending on its color. For this application, shorter light is reflected and longer light is transmitted by the splitter. Ploem placed the chromatic splitter in the optical path between the objective lens and the ocular, at a 45° angle, so that it would reflect shorter light downward toward the objective. The longer- fluorescence emission light would be transmitted through the chromatic beam splitter toward the ocular.

The microscopes that you have utilized in this and other courses all operate in the same general fashion. Light beams pass through a condenser lens system and provide illumination of an object at many points simultaneously. For incident light fluorescence microscopy, the objective lens also acts as a condenser for the excitation light beam. In its interaction with the object, some of this light is absorbed, some of this light is scattered, some of this light is reflected, and some of this light is slowed or retarded (relative to a beam of light that does not pass through the object). A portion of the light that has interacted with the object then passes through the imaging lens system of the microscope where it provides us with visual or pictorial image information about the object. Like the process of illumination, the process of image generation operates in a parallel fashion, where large numbers of light beams contribute to the image simultaneously. Resolution is limited by the closeness of overlapping points of brightness or darkness. In a practical sense, the limit of resolution is 0.18-0.2 µm with the best available objective lenses and a good specimen.

To observe cells with the fluorescence microscope, it is important to know the spectral characteristics of the fluorochrome that has been employed. In order to excite the fluorochrome properly and then observe its fluorescence emission, the appropriate filter packages must be present in the microscope. The fluorochrome may not fluoresce at all if the cells are illuminated with the inappropriate filter pack present in the optical path. Finally, for any kind of fluorescence localizations to be performed, it is essential to have the appropriate controls, to be sure that the cells do not exhibit excessive autofluorescence (that is, they do not glow in the absence of the fluorochrome), and that the fluorochrome is responsible for the localization pattern observed. In the laboratory, we have several microscopes equipped for incident light fluorescence microscopy.

Confocal Scanning Optical Microscopy

In the incident light fluorescence microscope, a light beam passes through a chromatic beam splitter and then the objective lens to illuminate a specimen. This light beam is used to excite electrons in fluorochrome molecules present in the object. As some of those excited electrons return to their ground state, the emission of light is detectable through the oculars of the microscope, or with a camera or video printer. The image is generated continuously, across the entire field of view. A primary problem with the fluorescence images generated in this way is that out-of-focus fluorescence appears as 'flare' in the object, and reduces the signal substantially. In addition, human eyes are not sufficiently sensitive photodetectors for the lowest levels of fluorescence, and most video-based imaging systems are only slightly better than your eyes. Under conditions where there is sufficient signal for you to easily observe fluorochrome distribution patterns, the excitation light can be of sufficient intensity to photooxidize (i.e., burn) your specimen. Much information can be lost with just a few seconds of exposure to the excitation lamp. The Confocal Scanning Optical Microscope, an expensive piece of instrumentation that illuminates the object with a small beam of light in a point-by-point (i.e., serial) fashion, eliminates most of the photoxidation problems, permitting the observation of objects for extended periods at very high resolution with little loss of signal. The placement of a small aperture in the beam path generates a small depth of field, and effectively eliminates out of focus information in image formation.

The confocal scanning optical microscope is designed to illuminate an object in a serial fashion, point by point, where a small beam of light (from a LASER) is scanned across the object rapidly in an X-Y raster pattern. The raster pattern can be created in several ways, but in one of the more popular instruments, it occurs as a consequence of the simultaneous rotation and vibration of a polygonal mirror. The vibration is caused by the activity of a servogalvanometer, while the rotation is caused by the activity of a small electric motor. Thus, a bright spot of light scans across an object from top to bottom, line by line. The image is also generated point-by-point. Image formation is translated into intensities at each spot in the X-Y raster by a photomultiplier tube. The intensity information is digitized and stored in a computer. A complex image processing software package permits visualization and manipulation of the images. Resolution is limited by spot size for the LASER and approaches 0.12-0.15 µm for an ideal specimen and with the best available objective lenses.

The manufacturers of confocal scanning optical microscopes include a pinhole diaphragm at a very special place in the optical path, near to the site of the photomultiplier tube. This pinhole is situated in a plane where the light from the in-focus part of the image converges to a point. Light from object planes above or below that of the focused image do not converge at the spot in the optical path occupied by the pinhole. Because of this design, out of focus image information is darkened to the extent that it is not detectable. The consequence is that all out of focus information is removed from the image and the confocal image is basically an 'optical section' of what could be a relatively thick object. The 'thickness' of the optical section may approach the limit of resolution, but in practice, the resolution in the Z-direction is somewhat greater, approximately 0.4-0.8 µm. The value of optical sectioning is best realized with fluorescence microscopy, where out-of-focus information alters, distorts, or even degrades the image. Because the confocal images are stored in a computer, it is possible to stack them up and generate three-dimensional reconstructions. The image processing programs also enable us to rotate these images and observe three-dimensional aspects of cellular structure. It may be clear to you that the computer responsible for these image manipulations must be fast and powerful. The biggest problem is one of image storage, where single images can routinely occupy >1,000,000 bytes of space. In rather short periods of use, it is easy to accumulate sufficient numbers of images to fill the largest of hard disks.

Two of the three the confocal scanning optical microscopes located on campus were manufactured by Carl Zeiss, located in Germany. The newest instrument (model 510) has three lasers and four photomultipliers and is designed so that we could illuminate with two or three colors of light in rapid succession and detect as many as three superimposed signals (essentially) simultaneously. The signals are separated from each other on the basis of color, using an acoustical optical tunable filter (AOTF). The optical microscope is an inverted stand. The most important operational difference between this microscope and the upright microscope in most laboratories is that with this instrument, the slide is placed in the stage holder upside-down. Like most modern research microscopes, this microscope is equipped for phase contrast, differential interference contrast and fluorescence microscopy and can be used with these imaging techniques for conventional imaging. However, it is equipped with a number of very highly corrected (read expensive) objective lenses attached to the turret, just below the stage. These lenses are necessary for high resolution confocal microscopy. The confocal part of this microscope is contained in a box that is attached to the inverted stand through an access port. As is the case with incident light fluorescence, the laser light passes through the objective lens to illuminate the specimen. An air suspension table is designed to eliminate vibrations present in the building.

Deconvolution Microscopy and Image Reconstruction

An alternative approach for eliminating flare from fluorescent image stacks is to perform intensive, iterative image analysis and processing, from objects that have been illuminated and photographed at multiple, adjacent focal planes. The images are obtained with a high-performance CCD camera, operating at very high magnification, using standard incident light fluorescence microscopy. The excitation source is a mercury arc lamp, and bandwidth for excitation and emission are controlled by filters placed in rotating filter wheels. The lamp is stabilized and the beam is randomized for uniform illumination of the specimen. Unlike confocal scanning instruments, the whole field of view is illuminated simultaneously with this microscope. It is possible to perform rapid sequential imaging (4 colors) from multiple fluorochromes with this microscope. At very high magnification, fluorescence from any spot in a cell acts as a point source. By knowing the image spread functions above and below the plane of focus, it is possible to determine points of origin for fluorescence, and spreading beams of light from that point source, above and below the plane of focus. An iterative algorithm, which is essentially a linear combination is performed by a computer on the adjacent pixels within a single image plane, and in successive image planes through the thickness of the object. Spreading light beams are subtracted from reconstructed image stack, and that light is added back to the source, thereby reducing noise and increasing signal, respectively. We have recently acquired a sophisticated DeltaVision microscope from Applied Precision, Inc., which is designed to acquire these images and then perform the computer-intensive operations. This kind of microscope is particularly well suited for generating three-dimensional fluorescence images from small, living cells.

Polarization Light Microscopy

When light passes through an object, it interacts with some or all of the atoms and molecules present in that object. In these interactions, sometimes light of a particular (i.e., color) is absorbed by the atoms or molecules, while sometimes light is scattered. The interaction of light with a translucent object often results in a slight reduction in the velocity of the light beam. The extent of this reduction in velocity can be measured as the refractive index of the object. For certain kinds of objects, especially those with high order in particular axes of the object, such a crystalline or paracrystalline arrays, the interaction with light beams is vastly different, depending on the orientation of the object relative to the impinging light beam. As a result, the refractive indices are measurably different in different axes of the object. Such an object with multiple refractive indices is termed birefringent. Birefringence (multiple refractive indices) results from the alignment of atoms or molecules in particular planes of an object these atoms or molecules interact strongly with light beams impinging on them from a particular direction, and to a far lesser extent with light beams impinging on them from a different direction. There are two kinds of birefringence, intrinsic birefringence, which results from atomic or molecular order in a crystalline or paracrystalline array (i.e., calcite crystals, membranes) and form birefringence, which results from supramolecular associations in paracrystalline arrays (i.e., microtubules in a spindle).


- Polarized Light and Birefringent Retardation -

Any light beam shining in a particular direction vibrates in all directions around the axis of travel. Light beams whose vibration has been restricted to a single plane, or to a few planes is known as polarized light. Birefringence is directly observable as differences in intensity in different axes of crystalline or paracrystalline objects when they are viewed with polarized light. Since birefringence results from differences in the number of interactions between the light beam and atoms or molecules in the object in different directions, in practice, the object is rotated around the plane of vibration for the polarized light beam to maximize the intensity differences in the object (usually, the dominant object axis is at a 45o angle relative to the plane of polarization). The extent of the difference in refractive indices in different axes of the object is a measurable quantity known as birefringent retardation (BR). BR is measured (as a distance) by placing an object with known birefringent retardation into the light beam, and, by rotating the calibrated object around the optic axis, extinguishing the brightness in the sample. Using this compensation technique, BR has been shown to be directly related to the number of aligned microtubules in mitotic spindles in living cells. This principle and procedure can be of importance in studying microtubule dynamics, where mitotic spindles of developing sea urchins can be visualized in a totally noninvasive way.


Stereo Dissecting Microscope Focusing

If you are trying to get a stereo microscope into focus, the body of the microscope is either too far away or too close to your sample. If you know the working distance for the stereo microscope, you can properly set up the microscope so the head is the correct distance from the stand. Working distance is the distance that is required between the lens of the stereo microscope body and the top of your sample in order for your sample to appear in focus when looking through the microscope.

Keep in mind that when you add or remove a stereo microscope auxiliary lens, the working distance of your stereo microscope will change as well.


Watch the video: 本気で眠りたいあなたへ聞き流し雑学音声分睡眠用寝落ち専用 (September 2022).


Comments:

  1. Tajo

    Bravo, you were visited with an excellent idea

  2. Juzilkree

    I do not think so.

  3. Zulut

    There is something in this and I think this is a great idea. I agree with you.

  4. Kamron

    I believe that you are wrong. I can prove it. Email me at PM, we will talk.

  5. Wilfrid

    It does not quite fit me.



Write a message