Continuous stomatal conductance measurements

Edaphic Scientific 2019 

Continuous stomatal conductance measurements

by Edaphic Scientific (2019)

With traditional instrumentation, stomatal conductance is difficult to measure. Traditional meters, such as a porometer, are slow and laborious. Typically, a single measurement can take several minutes and measuring many samples is very time consuming. Moreover, an instrument to measure stomatal conductance needs regular calibration and maintenance which just adds to the frustration of taking these very important physiological measurements.

Edaphic Scientific provides an easy-to-use and low maintenance solution for continuous stomatal conductance measurements. Stomatal conductance can be measured at a minimum of five-minute intervals but a single leaf can be measured continuously for several days to weeks.

As the sensor is connected to a data logger, measurements can be performed at any time of the day without the need for a researcher or technician to be present. With a modem connected to the data logger, stomatal conductance of a leaf can be viewed and monitored anywhere in the world with an internet connection.

A continuous data set of stomatal conductance over several days to weeks will provide important insights into the physiology of plants in response to experimental and environmental treatments.

the SF-4M sensor for stomatal conductance



Epidermal and cuticular mounts of plant material obtained by maceration

Epidermal and cuticular mounts of plant material obtained by maceration

by Kiger R. W. (1971)

Robert W. Kiger, University of Maryland, College Park (College Park, United States)


In Stain Technology, 46 (2): 71-75 – –


Mounts of leaf and stem epidermises or bare cuticles, useful in both general anatomical and specialized phylogenetic studies, can be prepared by a maceration process using Jeffrey’s solution (equal volumes of 10% aqueous CrO3 and 10% HNO3).

Leaves, including those of conifers, and stems with cuticles thick enough to maintain integrity when isolated are amenable to this process. Dried specimens are hydrated by boiling in water; fluid-preserved specimens are washed thoroughly in water; fresh specimens need no pretreatment. Specimens are cut to a convenient mount size and trimmed so as to allow adequate and even penetration of the macerating fluid. Laminar leaf segments are left with one edge untrimmed so that upper and lower epidermises remain contiguous.

Cylindrical leaf and stem segments are slit lengthwise through about half their thickness. Specimens are macerated in Jeffrey’s solution for 1 to 4 days until unwanted tissues are loosened and easily freed from the epidermis (or bare cuticle, if that is desired).

The macerating fluid is then washed out completely with changes of water and specimens are stained in a 0.5% aqueous solution of safranin. Dehydration is accomplished with several changes of tertiary butanol.

All unwanted tissues not removed by agitation during previous steps of the process are removed by teasing prior to mounting. Specimens are then mounted on slides in Canada balsam and dried in the usual manner.

Taking a silicone rubber plastic impression to form secondary transparent replicas to study stomata

A method of replicating dry or moist surfaces for examination by light microscopy

by Sampson J. A. (1961)

Joan Sampson

In Nature 191: 932–933 – –


The use of transparent replicas is a convenient method for the microscopic study of surfaces. Perfectly dry structures can be replicated with plastic substances such as ‘Collodion’, ‘Formvar’ or methacrylate, but a serious disadvantage to the general use of these materials is that they ‘mist’ when allowed to harden in a moist atmosphere.

Accordingly, they cannot be used satisfactorily with specimens that either become distorted when dry or, like many biological specimens, have a naturally wet surface.

The following method, which overcomes this difficulty, consists essentially of taking a primary impression of the surface with a silicone rubber plastic and using this to form secondary transparent replicas.

A fast method to measure stomatal aperture by MSER on smart mobile phone

A fast method to measure stomatal aperture by MSER on smart mobile phone

by Liu S., Tang J., Petrie P., Whitty M. (2016)

  • Scarlett Liu,
  • Julie Tang,
  • Paul Robert Petrie,
  • Mark Whitty,

In: Imaging and applied optics congress; 2016. p. 3–5 – –


A fast image processing method is proposed for detecting stomata and measuring stomatal aperture size in individual images. The accuracy of aperture measurements is 97%. A prototype mobile application is developed to assist field measurements.

Preparation of enzymatically cleaned and isolated stomata

Preparation of enzymatically cleaned leaf epidermal strips of Nicotiana glauca

by Hudson S.,  Trail J., Simmons D., Baldwin L., Myers R., Tom B., Mohr J., Tallman G. (1983)

Stephen Hudson, Jeff Trail, Dwayne Simmons, Larry Baldwin, Rebecca Myers, Barry Tom, Judy Mohr, Gary Tallman, 

Natural Science Division, Pepperdine University, Malibu, CA 90265 U.S.A.

In  Plant Sci Lett 32: 1-8 – 5 –


A technique for enzymatically cleaning leaf epidermal strips of Nicotiana glauca so that guard cells remain the only intact and viable cells is described.

The method relies on differential sensitivities of epidermal, mesophyll, and guard cell walls to digestion with a mixture of Cellulysin and hemicellulase.

Guard cells isolated by this procedure remain joined at their ends as duplexes, retain continuous cell walls, and are free of epidermal and mesophyll cell wall fragments and cytoplasmic debris. Yields range from 90–95% of original cells. All recovered cells concentrate neutral red and exclude trypan blue. In addition, duplexes isolated from either adaxial or abaxial surfaces show significant increases in width and aperture over dark controls when illuminated in solutions containing 30 mM KCl. Yields approach those necessary for standard methods of biochemical analysis. A brief comparison with existing techniques for guard cell isolation is included.

Preparation of leaf epidermis for study of topography and stomata

Preparation of leaf epidermis for topographic study

by Clarke J. (1960)

John Clarke,

In Stain Technol. 33: 35–39 – –


Epidermal strips of leaves of the Gramineae can be prepared using the following technique: The mature leaf is dipped in boiling water to kill the cells, and decolorized in boiling 70% alcohol. It is cleared and softened in 88% lactic acid. Epidermal, mesophyll and vascular tissue is removed from a selected constant area of the leaf leaving an epidermal strip 1-3 cm in length. This is inverted on a slide, stained in lactopheno-cotton blue, and destained in 88% lactic acid. Transverse and longitudinal sections of the strip are obtained at this stage. The epidermal strip is finally mounted on a slide in 88% lactic acid. The preparation is photographed with a 35 mm camera using transmitted light, and a yellow filter in the microscope lamp. Photomicrographs of known enlargement are then prepared from which accurate measurements can be recorded. The technique is applicable to both fresh and herbarium material.

Epidermal features and stomata in fossil plant impressions with SEM

The study of cuticular and epidermal features in fossil plant impressions using silicone replicas for scanning electron microscopy

by Moisan P. (2012)


In Palaeontologia Electronica 15(2): 1-9 –


FIGURE 3. 1. SEM image of latex replica of the herbaceous lycopsid Isoetites. Scale bar equals 250 μm. 2. SEM
image of VPS replica of the same specimen at the same magnification as shown in Figure 2.1., showing excellent
well-preserved epidermal cells. Scale bar equals 250 μm. 3. Detail of the Figure 2.1. Note that details of epidermal
cells are indistinguishable, and air bubbles are present over the surface. Scale bar equals 50 μm. 4. Detail of the Figure 2.2. Scale bar equals 50 μm. 5. SEM image of latex replica of the bennettitalean Pterophyllum pinnatifidum.
Deformation on the latex surface and air bubbles are present. Scale bar equals 100 μm. 6. SEM image of VPS replica of the same specimen at the same magnification as shown in Figure 2.5., showing intercostal field densely covered with papillae. Scale bar equals 100 μm. 7. Detail of Figure 2.5. Scale bar equals 25 μm. 8. Detail of Figure 2.6.,
showing a papillate surface. Scale bar equals 25 μm.