Measuring Fluxes of Mineral Nutrients and Toxicants in Plants with Radioactive Tracers

Devrim Coskun; Dev T. Britto; Ahmed M. Hamam; Herbert J. Kronzucker

doi:10.3791/51877

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Environment

Measuring Fluxes of Mineral Nutrients and Toxicants in Plants with Radioactive Tracers

Published: August 22, 2014

doi:

10.3791/51877

Devrim Coskun¹, Dev T. Britto¹, Ahmed M. Hamam¹, Herbert J. Kronzucker¹

¹Department of Biological Sciences,University of Toronto

Summary

In planta measurement of nutrient and toxicant fluxes is essential to the study of plant nutrition and toxicity. Here, we cover radiotracer protocols for influx and efflux determination in intact plant roots, using potassium (K⁺) and ammonia/ammonium (NH₃/NH₄⁺) fluxes as examples. Advantages and limitations of such techniques are discussed.

Abstract

Unidirectional influx and efflux of nutrients and toxicants, and their resultant net fluxes, are central to the nutrition and toxicology of plants. Radioisotope tracing is a major technique used to measure such fluxes, both within plants, and between plants and their environments. Flux data obtained with radiotracer protocols can help elucidate the capacity, mechanism, regulation, and energetics of transport systems for specific mineral nutrients or toxicants, and can provide insight into compartmentation and turnover rates of subcellular mineral and metabolite pools. Here, we describe two major radioisotope protocols used in plant biology: direct influx (DI) and compartmental analysis by tracer efflux (CATE). We focus on flux measurement of potassium (K⁺) as a nutrient, and ammonia/ammonium (NH₃/NH₄⁺) as a toxicant, in intact seedlings of the model species barley (Hordeum vulgare L.). These protocols can be readily adapted to other experimental systems (e.g., different species, excised plant material, and other nutrients/toxicants). Advantages and limitations of these protocols are discussed.

Introduction

The uptake and distribution of nutrients and toxicants strongly influence plant growth. Accordingly, the investigation of underlying transport processes constitutes a major area of research in plant biology and agricultural sciences^1,2, especially in the contexts of nutritional optimization and environmental stresses (e.g., salt stress, ammonium toxicity). Chief among methods for the measurement of fluxes in plants is the use of radioisotopic tracers, which was developed significantly in the 1950s (see e.g., ³) and continues to be widely used today. Other methods, such as measurement of nutrient depletion from the root medium and/or accumulation in tissues, use of ion-selective vibrating microelectrodes such as MIFE (microelectrode ion flux estimation) and SIET (scanning ion-selective electrode technique), and use of ion-selective fluorescent dyes, are also widely applied, but are limited in their ability to detect net fluxes (i.e., the difference between influx and efflux). The use of radioisotopes, on the other hand, allows the researcher the unique ability to isolate and quantify unidirectional fluxes, which can be used to resolve kinetic parameters (e.g., K_M and V_max), and provide insight into the capacity, energetics, mechanisms, and regulation, of transport systems. Unidirectional flux measurements made with radiotracers are particularly useful under conditions where the flux in the opposite direction is high, and the turnover of intracellular pools is rapid⁴. Moreover, radiotracer methods allow measurements to be conducted under fairly high substrate concentrations, unlike many other techniques (see ‘Discussion’, below), because the traced isotope is observed against a background of another isotope of the same element.

Here, we provide detailed steps for the radioisotopic measurement of unidirectional and net fluxes of mineral nutrients and toxicants in intact plants. Emphasis will be made on flux measurement of potassium (K⁺), a plant macronutrient⁵, and ammonia/ammonium (NH₃/NH₄⁺), another macronutrient which is, however, toxic when present at high concentrations (e.g., 1-10 mM)². We will use the radioisotopes ⁴²K⁺ (t_1/2 = 12.36 hr) and ¹³NH₃/¹³NH₄⁺ (t_1/2 = 9.98 min), respectively, in intact seedlings of the model system barley (Hordeum vulgare L.), in the description of two key protocols: direct influx (DI) and compartmental analysis by tracer efflux (CATE). We should note from the outset that this article simply describes the steps necessary to perform each protocol. Where appropriate, brief explanations of calculations and theory are provided, but detailed expositions of each technique’s background and theory can be found in several key articles on the subject^4,6-9. Importantly, these protocols are broadly transferable to flux analysis of other nutrients/toxicants (e.g., ²⁴Na⁺, ²²Na⁺, ⁸⁶Rb⁺, ¹³NO₃^–) and to other plant species, albeit with a few caveats (see below). We also stress the importance that all researchers working with radioactive materials must work under a license arranged through their institution’s ionizing radiation safety regulator.

Protocol

1. Plant Culture and Preparation

Grow barley seedlings hydroponically for 7 days in a climate-controlled growth chamber (for details, see ¹⁰).
NOTE: It is important to consider examining plants at a variety of developmental stages, as nutrient requirements will change with age.
One day prior to experimentation, bundle several seedlings together to make a single replicate (3 plants per bundle for DI, 6 plants per bundle for CATE). Bundle seedlings by wrapping a 2-cm piece of Tygon tubing around the basal portion of the shoots, and securing the tubing with tape to create a “collar”.
NOTE: The number of plants per bundle may vary based on experimental conditions ^10,13,14. Bundling is done to improve statistics and measuring accuracy, particularly when root mass and/or specific activity are low.

2. Preparation of Experimental Solutions/Materials

NOTE: The following is typically performed 1 day prior to experimentation.

For DI, gather the following: Pre-labeling, labeling, and desorption solutions (for details, see ¹¹), centrifugation tubes (for spin-drying of plant samples), and sample vials (for plant material and specific activity [S_o; see below]). Aerate and mix all solutions.
For CATE, gather the following: Well-mixed, aerated labeling and elution solutions (for details, see ¹⁰), efflux funnels, centrifugation tubes (for spin-drying of plant samples), and sample vials (for eluates, plant samples, and determination of S_o and dilution factor [D_f; see below]).

3. Prepare Radiotracer

CAUTION: The following safety steps should be taken prior to working with radioactivity.

Ensure that the requirements of the radioactive materials license are understood and followed. Wear proper safety equipment (i.e., goggles, gloves, lab coat, lead vest/collar) and dosimeters (e.g., TLD ring and badge). Set up shielding (i.e., Plexiglas and lead bricks) and perform radioactive work behind it. Ensure that a Geiger-Müller counter is present in order to routinely monitor for contamination.
Preparation of ⁴²K⁺
1. Place a clean, dry beaker on the balance. Zero the balance.
2. Remove vial of tracer (20 mCi of ⁴²K₂CO₃, in powder form) from packaging and pour tracer into the beaker. Take note of the mass.
3. Pipette 19.93 ml of dH₂O, followed by 0.07 ml of H₂SO₄, into the beaker. This will drive the following chemical reaction:
  ⁴²K₂CO₃(s) + H₂SO₄(l) + H₂O (l) → ⁴²K₂SO₄(l) + CO₂(v) + 2H₂O (l)
4. Calculate the concentration of the radioactive stock solution, given the mass and molecular weight of K₂CO₃, and the volume (20 ml).
  NOTE: If working with ¹³NH₃/¹³NH₄⁺ The tracer is produced in a cyclotron via the proton bombardment of the oxygen atom of water (typically resulting in 100-200 mCi activity; for production details, see ¹²). Because the quantity of ¹⁴NH₃/¹⁴NH₄⁺ is extremely low in these solutions, the N concentration of the stock solution is negligible.

4. Direct Influx (DI) Measurement

For ⁴²K⁺, pipette the amount of radioactive stock solution required to reach the desired final concentration of K⁺ into the labeling solution.
1. For ¹³NH₃/¹³NH₄⁺, pipette a small amount (<0.5 ml) into the labeling solution. Allow the labeling solution to mix thoroughly (via aeration).
Pipette a 1 ml sub-sample of labeling solution into a sample vial and repeat three times (4 samples in total).
1. Measure radioactivity in vials (in “counts per minute”, cpm), using a gamma counter. Ensure that the counter is programmed such that cpm readings are corrected for isotopic decay (this is particularly important for such short-lived tracers).
2. Calculate S_o (expressed as cpm µmol^-1) by averaging the counts of the four samples (cpm ml^-1) and dividing by the concentration of substrate in solution (µmol ml^-1).
Immerse roots in pre-labeling (non-radioactive) solution for 5 min, to pre-equilibrate plants under test conditions (see e.g., ^10,13,14 for variations in pre-label time).
Immerse roots in labeling (radioactive) solution for 5 min.
NOTE: Labeling times can vary based on experiment ^3,4,7-10.
Transfer roots to desorption solution for 5 sec to remove the bulk of surface-adhering radioactivity. Transfer roots into a second beaker of desorption solution for 5 min to further clear roots of extracellular tracer.
Dissect and separate shoots, basal shoots, and roots.
Place roots in centrifuge tubes and spin samples for 30 sec in a low-speed, clinical-grade centrifuge (~5,000 x g) to remove surface and interstitial water.
Weigh roots (fresh weight, FW).
Count radioactivity in plant samples (shoot, basal shoot, and root; see step 4.2.1).
Calculate the flux. Calculate influx into the plant using the formula
Φ = Q*/S_owt_L
where Φ is the flux (µmol g^-1 hr^-1), Q* is the quantity of tracer accumulated in tissue (cpm, usually in root, shoot, and basal shoot, combined), S_o is the specific activity of the labeling solution (cpm µmol^-1), w is the root fresh weight (g), and t_L is the labeling time (hr).
NOTE: More sophisticated calculation can be made to account for simultaneous tracer efflux from roots during labeling and desorption, based on parameters obtained from CATE (see below; for details, see ⁴).

5. Compartmental Analysis by Tracer Efflux (CATE) Measurement

Prepare labeling solution and measure S_o (see steps 4.1 – 4.2, above).
Measure dilution factor (D_f).
NOTE: Often, the position of the sample relative to the detector in the gamma counter can influence the quantity of radiation measured. See discussion for details.
1. After measuring S_o, add 19 ml of H₂O to each sample (such that final volume = eluate volume = 20 ml). Count radioactivity in each 20-ml sample (see step 4.2.1).
2. Calculate D_f by dividing the average cpm of the 1-ml samples by the average cpm of the 20-ml samples.
Immerse roots in labeling solution for 1 hr.
Remove plants from labeling solution and transfer plants to efflux funnel, ensuring all root material is within the funnel. Gently secure plants to side of efflux funnel by applying a small strip of tape over the plastic collar.
Gently pour the first eluate into the funnel. Start timer (counting up).
Open the spigot and collect the eluate in the sample vial after 15 sec (note: elution time will vary; see below). Close the spigot. Gently pour the next eluate into the funnel.
Repeat step 5.6 for the remainder of the elution series, which follows, from the first to the final eluate: 15 sec (four times), 20 sec (three times), 30 sec (twice), 40 sec (once), 50 sec (once), 1 min (25 times), for a total elution period of 29.5 min
NOTE: Desorption series can vary based on experimental conditions ^7-10,13,14.
Once elution protocol is complete, harvest plants (steps 4.6 – 4.8, above).
Count radioactivity in eluates and plant samples in the gamma counter (multiplying the reading for each eluate by D_f, see 5.2).
Plot tracer release (cpm g (root FW)^-1 min^-1) as a function of elution time. For steady-state conditions, perform linear regressions and calculations of fluxes, half-lives of exchange, and pool sizes (for details, see ^6-9).

Representative Results

Figure 1 shows isotherms found using the DI technique (with ¹³N), for the influx of NH₃ into roots of intact barley seedlings grown at high (10 mM) NH₄⁺, and either low (0.02 mM) or high (5 mM) K⁺. The isotherms display Michaelis-Menten kinetics when NH₃ fluxes are plotted as a function of external NH₃ concentration ([NH₃]_ext; adjusted by changes in solution pH¹³). NH₃ fluxes were significantly higher at low K⁺ than at high K⁺. Analysis of Michaelis-Menten kinetic parameters showed that the K_M remained relatively stable between K⁺ levels (150 vs. 90 µM at low and high K⁺, respectively), while V_max is strongly reduced at high K⁺ (205 vs. 80 µmol g^-1 hr^-1). Thus, the data indicate that K⁺ level regulates nitrogen transport (V_max effect), but not by direct competition between K⁺ and NH₃ for binding sites of transporters (K_M effect). Rather, K⁺ may regulate NH₃ fluxes by other means, such as through modulation of aquaporin activity (for details, see ¹³).

DI is also useful for the capturing of relatively fast changes in influx due to nutritional shifts, or to the application of pharmacological agents. For example, Figure 2 highlights the rapid plasticity of the K⁺-uptake system in roots of intact barley seedlings grown at moderate (0.1 mM)-K⁺and high (10 mM)-NH₄⁺ conditions. Here, we observed a ~350% increase in K⁺ influx within 5 min of NH₄⁺ withdrawal from the external solution. This “ammonium withdrawal effect” (“AWE”) was found to be sensitive to the K⁺-channel blockers tetraethylammonium (TEA⁺), barium (Ba²⁺), and cesium (Cs⁺). Using DI and electrophysiological measurements in several Arabidopsis genotypes, we were able to conclusively ascribe the vast majority of the AWE to changes in activities of the Arabidopsis K⁺ channel, AtAKT1, and high-affinity K⁺ transporter, AtHAK5¹⁴.

Figure 3 plots the steady-state efflux of ⁴²K⁺, over time, from roots of pre-labeled barley seedlings grown at low (0.1 mM) K⁺ and moderate (1 mM) NO₃^–. These traces show how the CATE method can reveal rapid and significant changes in efflux upon application of various pharmacological/nutritional agents. Substantial, immediate inhibition of K⁺ efflux was observed upon either an application of 10 mM Cs⁺, a K⁺-channel blocker, or a sharp increase in K⁺ provision (from 0.1 to 10 mM). These results are consistent with molecular studies describing the unique gating properties of outward-rectifying K⁺ channels¹⁵_.By contrast, application of 10 mM NH₄⁺ rapidly and strongly stimulated K⁺ efflux. This effect can be explained by the activation of outward-rectifying K⁺ channels via depolarization of the electrical potential gradient across the plasma membrane of root cells¹⁶, which is known to occur upon introduction of NH₄⁺¹⁷. Thus, using this method, we have been able to demonstrate, in planta, that K⁺ channels mediate K⁺ efflux in roots of barley¹⁰.

Lastly, Table 1 shows CATE parameters extracted from measurements of steady-state ⁴²K⁺ efflux ([K⁺]_ext = 0.1 mM) in barley seedlings grown either with 1 mM NO₃^– or 10 mM NH₄⁺, the latter representing a toxic scenario. The high NH₄⁺ condition brings about a suppression of all K⁺ fluxes, and a significant decline in cytosolic K⁺ concentration ([K⁺]_cyt), which is normally homeostatically maintained at ~100 mM under healthy growth conditions¹⁸ (as observed, e.g., in Table 1, under NO₃^– supply).

Figure 1. ¹³NH₃ influx isotherms reveal how K⁺ supply regulates nitrogen transport. NH₃ influx as a function of varying external concentrations of NH₃([NH₃]_ext) in intact roots of barley seedlings grown at high (10 mM) NH₃/NH₄⁺ and either low (0.02 mM, red) or high (5 mM, blue) K⁺. Michaelis-Menten analyses of isotherms reveal that high-K⁺ provision has relatively little effect on the substrate affinity (i.e., K_M) of NH₃-uptake transporters, but significantly reduces the transport capacity (i.e., V_max; see ‘Representative Results’). Note, changes in [NH₃]_ext were established by shifting the external solution pH with NaOH, and thus the NH₃:NH₄⁺ ratios, as per the Henderson-Hasselbalch equation. Error bars indicate SEM of 4-7 replicates. (Reproduced from Coskun et al. Rapid ammonia gas transport accounts for futile transmembrane cycling under NH₃/NH₄⁺ toxicity in plant roots. Plant Physiol. 163, 1859-1867 (2013).)

Figure 2. NH₄⁺ withdrawal significantly stimulates channel-mediated K⁺ influx. K⁺ influx at steady state, and upon withdrawal of NH₄⁺, in roots of intact barley seedlings grown at low (0.1 mM) K⁺ and high (10 mM) NH₄⁺. The effect of K⁺-channel blockers (10 mM TEA⁺, 5 mM Ba²⁺, and 10 mM Cs⁺) on the stimulated K⁺ influx is pronounced. Asterisks denote different levels of significance between -NH₄⁺ and treatment pairs (*0.01 < P < 0.05, ***P < 0.001; one-way ANOVA with Dunnett’s multiple comparison post-hoc test). Asterisks in parentheses denote level of significance between control and -NH₄⁺ pair (Student’s t-test). Error bars indicate SEM of >4 replicates. (Reproduced from Coskun et al. Capacity and plasticity of potassium channels and high-affinity transporters in roots of barley and Arabidopsis. Plant Physiol. 162, 496-511 (2013).)

Figure 3. K⁺ efflux is channel-mediated under low-K⁺ conditions. Steady-state ⁴²K⁺ efflux in roots of intact barley seedlings grown at low (0.1 mM) K⁺ and moderate (1 mM) NO₃^–, and the immediate effects (at t = 15.5 min; see arrow) of 10 mM CsCl, 5 mM K₂SO₄, and 5 mM (NH₄)₂SO₄ on efflux. Each plot represents the mean of 3-13 replicates (SEM <15% of the mean). (Reproduced from Coskun et al. Regulation and mechanism of potassium release from barley roots: an in planta ⁴²K⁺ analysis. New Phytol. 188, 1028-1038 (2010).)

[K⁺]_ext	N source	Influx	Efflux	Net Flux	E:I Ratio	Pool Size	Half-life
(mM)	(mM)	(µmol g^-1 hr^-1)			E:I Ratio	(mM)	(min)
0.1	1 NO₃^–	7.22 ± 0.23	1.86 ± 0.18	5.36 ± 0.18	0.25 ± 0.02	98.84 ± 14.08	28.18 ± 3.40
0.1	10 NH₄⁺	1.89 ± 0.13	0.57 ± 0.05	1.32 ± 0.10	0.30 ± 0.01	28.39 ± 3.40	32.50 ± 4.69

Table 1. Steady-state K⁺ fluxes and compartmentation under various N provisions. Steady-state flux and compartmental analysis of barley seedlings grown at 0.1 mM K⁺, and either moderate NO₃^– (1 mM, as Ca²⁺ salt) or high NH₄⁺ (10 mM, as SO₄^2- salt). Errors indicate ± SEM of >8 replicates. (Reproduced from Coskun et al. Regulation and mechanism of potassium release from barley roots: an in planta ⁴²K⁺ analysis. New Phytol.188, 1028-1038 (2010) and Coskun et al. Capacity and plasticity of potassium channels and high-affinity transporters in roots of barley and Arabidopsis. Plant Physiol.162, 496-511 (2013).)

Discussion

As demonstrated in the examples above, the radiotracer method is a powerful means of measuring unidirectional fluxes of nutrients and toxicants in planta. Figure 1 shows that NH₃ influx can reach in excess of 225 µmol g^-1 hr^-1, which is perhaps the highest bona fide transmembrane flux ever reported in a plant system¹³, but the magnitude of this flux would not be visible if only net fluxes were measured. This is because a large efflux of NH₃ occurs at the same time as influx, in a futile cycling scenario that can result in a pronounced underestimate of influx that increases with labeling time¹³. By supplementing the tracer technique with electrophysiological analysis, we were able to demonstrate that under the conditions of Figure 1, both influx and efflux of ¹³N is primarily of the neutral gas NH₃, and not of its conjugate acid NH₄⁺(for details, see ¹³). This is the first in planta demonstration of rapid NH₃ gas fluxes in roots, and as such, provides important preliminary evidence towards unraveling the transport mechanism that lies at the heart of NH₃/NH₄⁺ toxicity in higher plants^2,13. Molecular work in heterologous expression systems has demonstrated that NH₃ can flow via aquaporins in plants¹⁹, and the data from Figure 1, along with recent pharmacological evidence, has begun to corroborate such findings at the level of the intact organism¹³.

Figures 2 and 3 also provide excellent examples of the utility of measuring unidirectional fluxes with radiotracers. Using DI with ⁴²K⁺, we were able to demonstrate that ion channels are not responsible for steady-state K⁺ uptake in roots of barley seedlings grown at low K⁺ and high NH₄⁺, in contrast to the model system Arabidopsis¹⁴. Only when NH₄⁺ was withdrawn did we see evidence for the engagement of K⁺ channels (Figure 2). Although the net flux of K⁺ is also stimulated by NH₄⁺ withdrawal (as shown by increased tissue K⁺ content¹⁴), only by measuring unidirectional influx were we able reveal the magnitude and rapid onset of this phenomenon. Moreover, by conducting DI measurements with mutants and pharmacological agents, we were able to identify which transport proteins were involved. Similarly, by applying nutritional and pharmacological agents while monitoring tracer efflux (Figure 3), we were able to characterize and identify mechanisms of K⁺ efflux from barley root cells¹⁰. Thus, techniques such as DI and CATE can be instrumental to the understanding of transport characteristics for a critical macronutrient.

As noted in the protocol, often the position of the sample relative to the detector in the gamma counter can influence the quantity of radiation measured. Thus, if a 1-ml sample is “topped up” with 19 ml of H₂O, the counts measured (cpm) in the 20-ml sample can be significantly lower than in the 1-ml sample, despite having the same amount of radiotracer. Therefore, a D_f can be applied to correct for this apparent ‘dilution’ of radioactivity. This issue is often not explicitly stated by manufacturers of detection instrumentation and must be worked out by the individual researcher. Similarly, the effectiveness of shielding within detectors against ambient radiation (i.e., from nearby samples within the counter) can be exaggerated by manufacturers, and such issues should be worked out for individual measuring systems.

A major advantage of the tracer technique is its non-invasiveness, which provides a means to measure fluxes, intracellular pool sizes, and exchange rates, under steady-state conditions. For example, with CATE, we could non-invasively quantify cytosolic concentrations of K⁺ (Table 1). This can be preferable to alternative methods such as impalement of cells with ion-selective microelectrodes¹⁸, which imparts physical and possibly chemical disturbances to the cell. In addition, the tracer technique is unique in that it provides a comprehensive view of fluxes and compartmentalization for whole organs and intact plants. This is important if one is interested in understanding whole-plant nutrient dynamics, toxicity, and ultimately, performance in the field. Lastly, radiotracer methods allows for very sensitive measurements to be conducted under fairly high substrate concentrations. Traditional depletion experiments and microelectrode techniques can experience issues of background interference and thus, may require that the external concentration of the substrate of interest is lowered well below that provided during growth. This could be problematic if one is interested in studying “steady-state” conditions of high substrate concentrations (such as with NH₃/NH₄⁺ toxicity or “high-K⁺” conditions; see above).

It should be noted that, like all techniques, measuring fluxes with radiotracers is not without its limitations. For example, the availability of radiotracers can be problematic, particularly for very short-lived isotopes like ¹³N that require close proximity to a production facility such as a cyclotron. Another major limitation is that at times, it can be difficult to discriminate between fluxes that are occurring across membranes and those occurring extracellularly. Such distinctions call for rigorous phase testing^7,10,20. In the case of K⁺ efflux, only after careful examination were we able to confirm that steady-state ⁴²K⁺ release from roots was occurring not across cell membranes at high [K⁺]_ext (>1 mM)¹⁰, but from extracellular spaces (c.f., Figure 3). Such issues can be resolved by examining the effect of a wide range of pharmacological agents, or through thermodynamic analyses, which have shown, for example, that very high Na⁺ fluxes reported under saline conditions would be energetically unfeasible were they to proceed across cell membranes^21,22.

Disclosures

The authors have nothing to disclose.

Acknowledgements

This work was supported by the Natural Sciences and Engineering Council of Canada (NSERC), the Canada Research Chair (CRC) program, and the Canadian Foundation for Innovation (CFI).

Materials

Name of Material/ Equipment	Company	Catalog Number	Comments/Description
Gamma counter	Perkin Elmer		Model: Wallac 1480 Wizard 3"
Geiger-Müller counter	Ludlum Measurements Inc.		Model 3 survey meter
400-mL glass beakers	VWR	89000-206	For pre-absorption, absorption, and desorption solutions
Glass funnel	VWR	89000-466	For efflux funnel
Large tubing	VWR	529297	For efflux funnel
Medium tubing	VWR	684783	For bundling
Small tubing	VWR	63013-541	For aeration
Aeration manifold	Penn Plax Air Tech	vat 5.5	To control/distribute pressurized air into solutions
Glass scintillation vials	VWR	66022-128	For gamma counting
Glass centrifuge tubes	VWR	47729-576	For spin-drying root samples
Kimwipes	VWR	470173-504	For spin-drying root samples
Dissecting scissors	VWR	470001-828
Forceps	VWR	470005-496
Low-speed clinical centrifuge	International Equipment Co.	76466M-4	For spin-drying root samples
1-mL pipette	Gilson	F144493
10-mL pipette	Gilson	F144494
1-mL pipette tips	VWR	89079-470
10-mL pipette tips	VWR	89087-532
Analytical balance	Mettler toledo	PB403-S/FACT

References

Kronzucker, H. J., Coskun, D., Schulze, L. M., Wong, J. R., Britto, D. T. Sodium as nutrient and toxicant. Plant Soil. 369, 1-23 (2013).
Britto, D. T., Kronzucker, H. J. NH4+ toxicity in higher plants: a critical review. J. Plant Physiol. 159, 567-584 (2002).
Epstein, E. Mechanism of ion absorption by roots. Nature. 171, 83-84 (1953).
Britto, D. T., Kronzucker, H. J. Can unidirectional influx be measured in higher plants? A mathematical approach using parameters from efflux analysis. New Phytol. 150, 37-47 (2001).
Britto, D. T., Kronzucker, H. J. Cellular mechanisms of potassium transport in plants. Physiol. Plant. 133, 637-650 (2008).
Walker, N. A., Pitman, M. G., Lüttge, U., >Pitman, M. .. G. Measurement of fluxes across membranes. Encyclopedia of plant physiology. 2 Part A, (1976).
Kronzucker, H. J., Siddiqi, M. Y., Glass, A. D. M. Analysis of 13NH4+ efflux in spruce roots – A test case for phase identification in compartmental analysis. Plant Physiol. 109, 481-490 (1995).
Siddiqi, M. Y., Glass, A. D. M., Ruth, T. J. Studies of the uptake of nitrate in barley. 3. Compartmentation of NO3-. J. Exp. Bot. 42, 1455-1463 (1991).
Lee, R. B., Clarkson, D. T. Nitrogen-13 studies of nitrate fluxes in barley roots. 1. Compartmental analysis from measurements of 13N efflux. J. Exp. Bot. 37, 1753-1767 (1986).
Coskun, D., Britto, D. T., Kronzucker, H. J. Regulation and mechanism of potassium release from barley roots: an in planta 42K+ analysis. New Phytol. 188, 1028-1038 (2010).
Britto, D. T., Kronzucker, H. J., Maathuis, F. .. J. .. M. .. ,. Fluxes measurements of cations using radioactive tracers. Plant Mineral Nutrients: Methods and Protocols, Methods in Molecular Biology. Volume 953, 161-170 (2013).
Meeks, J. C., Knowles, R. ,., Blackburn, T. .. H. 13N techniques. Nitrogen isotope techniques. , 273-303 (1993).
Coskun, D., Britto, D. T., Li, M., Becker, A., Kronzucker, H. J. Rapid ammonia gas transport accounts for futile transmembrane cycling under NH3/NH4+ toxicity in plant roots. Plant Physiol. 163, 1859-1867 (2013).
Coskun, D., Britto, D. T., Li, M., Oh, S., Kronzucker, H. J. Capacity and plasticity of potassium channels and high-affinity transporters in roots of barley and Arabidopsis. Plant Physiol. 162, 496-511 (2013).
Johansson, I., et al. External K+ modulates the activity of the Arabidopsis potassium channel SKOR via an unusual mechanism. Plant J. 46, 269-281 (2006).
Nocito, F. F., Sacchi, G. A., Cocucci, M. Membrane depolarization induces K+ efflux from subapical maize root segments. New Phytol. 154, 45-51 (2002).
Wang, M. Y., Glass, A. D. M., Shaff, J. E., Kochian, L. V. Ammonium uptake by rice roots. 3. Electrophysiology. Plant Physiol. 104, 899-906 (1994).
Walker, D. J., Leigh, R. A., Miller, A. J. Potassium homeostasis in vacuolate plant cells. Proc. Natl. Acad. Sci. U.S.A. 93, 10510-10514 (1996).
Holm, L. M., et al. NH3 and NH4+ permeability in aquaporin-expressing Xenopus oocytes. Pflugers Archiv. Eur. J. Physiol. 450, 415-428 (2005).
Britto, D. T., Kronzucker, H. J. Trans-stimulation of 13NH4+ efflux provides evidence for the cytosolic origin of tracer in the compartmental analysis of barley roots. Funct. Plant Biol. 30, 1233-1238 (2003).
Malagoli, P., Britto, D. T., Schulze, L. M., Kronzucker, H. J. Futile Na+ cycling at the root plasma membrane in rice (Oryza sativa L.): kinetics, energetics, and relationship to salinity tolerance. J. Exp. Bot. 59, 4109-4117 (2008).
Kronzucker, H. J., Britto, D. T. Sodium transport in plants: a critical review. New Phytol. 189, 54-81 (2011).

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Coskun, D., Britto, D. T., Hamam, A. M., Kronzucker, H. J. Measuring Fluxes of Mineral Nutrients and Toxicants in Plants with Radioactive Tracers. J. Vis. Exp. (90), e51877, doi:10.3791/51877 (2014).

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