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Chlorophyll a Fluorescence Parameters of Hulled and Hull-less Barley (Hordeum vulgare L.) DH Lines Inoculated with Fusarium culmorum
The Plant Pathology Journal 2019;35:112-124
Published online April 30, 2019
© 2019 The Korean Society of Plant Pathology.

Tomasz Warzecha1,* , Edyta Skrzypek2, Tadeusz Adamski3, Maria Surma3, Zygmunt Kaczmarek3, and Agnieszka Sutkowska1

1University of Agriculture in Kraków, Department of Plant Breeding and Seed Science Łobzowska 24, 31-140 Kraków, Poland, 2Polish Academy of Sciences, The Franciszek Górski Institute of Plant Physiology, Niezapominajek 21, 30-239 Kraków, Poland, 3Institute of Plant Genetics, Polish Academy of Sciences, Strzeszyńska 34, 60-681 Poznań, Poland
Correspondence to: *Phone) +48-12-6333606 ext.111, FAX) +48-12-6333606 ext.129, E-mail)
Received July 4, 2018; Revised October 17, 2018; Accepted February 12, 2019.
This is an Open Access article distributed under the terms of the Creative Commons Attribution Non-Commercial License ( which permits unrestricted noncommercial use, distribution, and reproduction in any medium, provided the original work is properly cited.

Barley worldwide is affected seriously by Fusarium seedling blight (FSB) and Fusarium head blight (FHB) diseases caused by the Fusarium species. The objective of this study was to facilitate the resistance of hulled and hull-less barley at different growth stages to F. culmorum according to direct parameters: disease rating (DR), fresh weight of leaves and roots, kernel weight per spike, kernel number per spike, plump kernels, and indirect parameters - chlorophyll a fluorescence (CF). Plate assay, greenhouse and field tests were performed on 30 spring barley doubled haploid (DH) lines and their parents infected with Fusarium culmorum. Direct parameters proved that hulled genotypes show less symptoms. Most studied chlorophyll a fluorescence (CF) parameters (apart from DIo/CS – amount of energy dissipated from PSII for laboratory test, TRo/CS – amount of excitation energy trapped in PSII reaction centers, ETo/CS – amount of energy used for electron transport and RC/CS – number of active reaction centres in the state of fully reduced PSII reaction center in field experiment) were significantly affected by F. culmorum infection. In all experiments, hulled genotypes had higher values of CF parameters compared to hull-less ones. Significant correlations were detected between direct and indirect parameters and also between various environments. It was revealed that ABS/CS, TRo/CS, and RC/CS have significant positive correlation in greenhouse test and field experiment. Significant correlations suggest the possibility of applying the CF parameters in selection of barley DH lines resistant to F. culmorum infection.

Keywords : chlorophyll a fluorescence, fungal infection, Fusarium head blight, Fusarium seedling blight, spring barley
Materials and Methods

Plant material

Material for the study included 32 spring barley (Hordeum vulgare L.) lines: 2 parental genotypes (hull-less line 1N86 and hulled line RK63/1), and 30 doubled haploid (DH) lines derived from F1 hybrids RK63/1 × 1N86. The parental lines differ in susceptibility to Fusarium culmorum infection. Line 1N86 was considered susceptible and RK63/1 resistant (Warzecha et al., 2015). DH lines generated from the crossing of 1N86 and RK63/1 were developed by the Hordeum bulbosum technique. Standard procedures were applied for crossing H. vulgare with H. bulbosum and in vitro culture of immature embryos (Kasha and Kao, 1970; Pickering and Devaux, 1992).

Plate assay

Inoculation of semi-germinated seeds was performed with an isolate of Fusarium culmorum (Plant Breeding Institute, Wageningen, Holland) culture in Petri dishes on a PDA medium (Potatoe Dextrose Agar – Sigma) at a temperature of 22°C without access to light, in a microbiological incubator (B 6060 Heraeus, USA) over a period of seven days. The kernels were surface disinfected for 15 min with 20% Domestos solution (commercial bleach, with sodium hypochlorite as the active ingredient) and substantially washed three times in sterile water and placed on blotting paper for 24 h for germination. Then the semi-germinated seeds were transferred onto PDA medium discs (ø 4 mm) overgrown with Fusarium culmorum mycelium. Barley kernels placed on sterile medium discs were the control. The test was repeated three times in February 2013. In each test 20 grains of each genotype were sown on Petri dishes for control and inoculated combinations. Therefore, the replication was a set of 20 plants of the same genotype. The assay for resistance was carried out in an airconditioned chamber over a period of 7 days at 22°C/20°C (day/night), with 130 μE/m2/s lighting, 12/12 h photoperiod and 100% relative humidity. To determine the effect of infection on seedling development, direct assessment using a disease rating (DR) (Chełkowski and Mańka, 1983) was calculated according to the formula:



  • ni – the number of plants of the ith category,

  • ith category – certain value from the 0–5 scale assessed by visual symptoms of disease where 0- no symptoms, 5 complete damage (over 80% of organ is damaged)

  • Di – numerical value of the ith category (ranged between 0–5),

  • N– the total number of plants in the sample,

  • Dmax – is the maximum value in 0–5 disease scale, Wojciechowski et al. (1997).

Chlorophyll fluorescence parameters were measured on the fully developed leaves of 7-day seedlings. The fresh weight (FW, mg) of leaves and roots of inoculated and control seedlings was also determined in each replication.

Production of inoculums for greenhouse and field test

The 300 ml Erlenmeyer flasks were filled with 50 g of wheat grain and 15 ml of water (40% moisture). After 24 h, they were autoclaved for 30 min at 1 atm. at a temperature of 121°C and then cooled. Fusarium culmorum isolate derived from SNA (Synthetic Nutrient Agar medium) medium (Chełkowski and Mańka, 1983) were transferred into the Erlenmeyer flasks (250 ml).

The methods of infection

After transferring on SNA slants, mycelium grew in 2–3 days, then was eluted with 1–2 ml of sterile water, mixed, scraped from the surface of the SNA slant and poured on the grain surface.

After inoculation, the flasks were incubated at a temperature of 22°C without access to light, in a microbiological incubator (B 6060 Heraeus, USA) and every second day were shaken in order to infect all grains uniformly. Inoculum production lasted approximately 3–4 weeks.

Preparation of inoculum to infect kernels

The spores were eluted with sterile water and filtered through several layers of gauze. Spore concentration was determined in a Neubauer chamber. The spore suspension was appropriately diluted to a concentration of 5 × 106 spores/ml.

Greenhouse test
Inoculation of kernels

Grains were soaked in a 5% solution of carboxymethylcellulose as a superadsorbent agent it adheres to the grains by dipping or coating. Grains were dried on Petri dish, and afterwards obtained a dry gel coating. After drying, coated grains were soaked for 1 h in a spore suspension – 10 ml per plate and shaken every five minutes. Control grains were soaked in sterile water.

Grains were dried at room temperature for 12 h and then sown in pots with sterile soil (Arseniuk et al., 1993).

The greenhouse assay for resistance was carried out at 18/13°C day/night, a photoperiod of 16/8 h light/darkness, and a light intensity 350 μE/m2/s.

In each combination (inoculated and control) 20 grains of each genotype were sown in sterile soil in three replications (altogether sixty grains of each line). One replication was a set of 20 plants of the same genotype.

Chlorophyll fluorescence was measured on the fully developed leaves of 14-day seedlings. After two weeks the plants were removed from the soil and necrosis or leaf discoloration, fresh weight of leaves (FW) and DR of leaves were determined in control and inoculated plants.

To determine the effect of infection on plant development under greenhouse conditions, the disease rating was calculated according to the formula given above, as described for plate assay resistance.

Field test

Field experiments were carried out in Prusy, South Poland (20°05′E 50°05′N). The average weather conditions (temperature and rain fall) during the vegetation season was as follows: March −0.9°C, 32.3 mm; April 8.8°C, 20.1 mm; May 14.2°C, 98.8 mm; June 17.6°C, 213.1 mm; July 19.2°C, 27.2 mm. The weather records were obtained from the weather station next to the experimental plots. The experiment with 32 genotypes and 2 treatments (inoculation and control) was carried out in a randomized block design. The experimental area was divided into 2 large plots (LP, one for control and one for inoculation. Each LP was divided into three blocks, one block was one replication and genotypes were randomly distributed inside each block. In each plot inside the block, seeds were sown in six 2-m rows, 20 cm apart, and 200 seeds in each row.

Each line was artificially inoculated with F. culmorum. At full anthesis (Zhadoks scale 67), 40 spikes of each line in each replication were sprayed (each spike separately) with 2 ml of conidial suspension (5 × 106 in 1 ml) of F. culmorum (W.G.Sm) Sacc., isolate KF350 (IPO348-01, ITEM6249) (Warzecha et al., 2010).

Chlorophyll a fluorescence parameters were measured on flag leaves two weeks after inoculation. DR of heads, kernel weight per spike (KWS), kernel number per spike (KNS) and kernel fractions: > 2.5 mm (KD1). 2.5-2.2 mm (KD2) and < 2.2 mm (KD3), in %) were examined in control and inoculated plants.

Chlorophyll a fluorescence parameters

Chlorophyll a fluorescence parameters were measured using a fluorometer (Handy PEA; Hansatech Instruments, King’s Lynn, Norfolk, UK) at 24°C after 20 min for the detached leaves to adapt to the dark conditions. The measurements were done using a saturating pulse of 3 000 μmol/m2/s, pulse duration of 1 s, and fixed gain (1.0×). Leaves of three plants of each line were measured in each block. The fluorescence intensity is measured and expressed in relative units. The Kautsky curve or chlorophyll fluorescence transient describes the fluorescence response change over time (Force et al., 2003). Using input data from the fluorescence transient, a group of fluorescence parameters, called the JIP-test, that quantify the stepwise flow of energy through Photosystem II was formulated by Strasser and Strasser (1995).

The following parameters were calculated: light energy absorption (ABS/CS), amount of excitation energy trapped in PSII reaction centers (TRo/CS), amount of energy used for electron transport (ETo/CS), amount of energy dissipated from PSII (DIo/CS), equal to [ABS/CS – TRo/CS]), number of active reaction centres in the state of fully oxidized PSII reaction center (RC/CSo), number of active reaction centres in the state of fully reduced PSII reaction center (RC/CS) (Czyczyło-Mysza et al., 2013; Strasser and Tsimillini-Michael, 1998; Strasser et al., 2000).

Statistical analysis

For the examined parameters, a two-way analysis of variance using the independent system was conducted. The distinguished sources of variability were tested using the fixed model. The evaluation of the correlations between characteristics was performed on the basis of the Pearson linear correlation coefficient. Statistical analysis was performed with the application of Statistica StatSoft, Inc.


The impact of F. culmorum infection was significant for most of the studied chlorophyll fluorescence (CF) parameters (apart from DIo/CS for laboratory test, ETo/CS and RC/CSo in field experiment) (Tables 1, 2). A significant influence of genotype on chlorophyll fluorescence parameters in all three experiments (plate assay, greenhouse and field tests) was also recorded. Treatment × genotype interaction was important mainly for CF parameters measured in the plate assay and greenhouse test, whereas for the field experiment this interaction was significant (at P < 0.05) only for Dlo/CS. In Supplementary Table 1–3 the mean values of CF are given for individual lines in control and infected plants. The impact of F. culomurm infection was also observed on direct parameters in greenhouse and field tests (Table 2). Infection significantly influenced the examined traits under greenhouse (DR and FW) and field (KNS, KWS, KD1, KD2, KD3) conditions (Table 2, Supplementary Table 2, 4). A significant impact of genotype on studied traits (except DR in field test) was also observed, while interaction between treatment and genotype was significant only for KD3 (Table 2).

In all experiments hulled genotypes had higher values of all measured CF parameters compared to hull-less ones (Supplementary Table 1–3). These data correspond with direct parameters, where hulled genotypes showed less disease symptoms. Estimates of differences between hulled and hull-less lines showed that infected hulled lines have had significantly (at P < 0.05) higher values of CF parameters in the plate assay (except Dlo/CS) and the greenhouse test (with an exception for Dlo/CS and RC/CSo), while in control plants these differences were not significant in greenhouse and field tests (Table 3, Supplementary Table 1).

The relationship observed between CF parameters and DR and FW of leaves and roots in the plate assay are presented in Table 4. In most cases (apart from DIo/CS) CF parameters had a significant negative correlation with DR of leaves and roots, which indicates that CF parameters decreased after inoculation. Higher values of DR resulted in lower performance of the PSII photosystem as its components are affected by infection. In contrast, the fresh weight of leaves had significant positive correlation with ETo/CS, RC/CSo and RC/CS, while the fresh weight of roots has significant positive correlation with ETo/CS. It is worth noting that ETo/CS was correlated with all direct parameters, negatively with DR of leaves and roots and positively with fresh weight of leaves and roots, both in control and inoculated plants (Table 4).

Correlation coefficients calculated for the greenhouse experiment revealed significant negative relations of all the studied CF parameters and DR of leaves for control and inoculated plants, but in infected plants the relation is much stronger (Table 5). When considering the fresh weight of leaves, the correlation coefficients are positive and significant both for control and infected plants.

Correlation coefficients between CF parameters and the direct traits observed in the field test (DR of head, number of kernel per head, weight of grains per head, kernel fractions (KD 1, KD2, KD3) showed that the most informative was DIo/CS (Table 6, Supplementary Table 4). This parameter had significant negative correlation with DR of head and the smallest grain fraction (KD1) and significant positive correlation with grain fraction KD3.

Data concerning the compatibility of CF parameters after inoculation assessed under various environments could provide useful information on whether plants express the same level of resistance in various conditions and various growth stages (Table 7). A significant positive correlation was revealed for a number of active reaction centers both oxidized and reduced (RC/CSo, RC/CS, respectively) between 7-day seedlings in the plate test and 14-day seedlings in the greenhouse test. Additionally, significant positive correlation was observed for light energy absorption (ABS/CS), amount of excitation energy trapped in PSII reaction centers (TRo/CS) and number of oxidized active reaction centers (RC/CSo) between 14-day seedlings grown in a greenhouse test and plants at field test.


Fusarium culmorum along with Microdochium nivale and M. majus are major agents responsible for seedling blight and root rot as well as Fusarium head blight in barley and wheat. Seedling blight can significantly reduce seedling emergence and establishment as a result of infection, especially under high soil moisture favourable for fungi development, Fusarium head blight can result in notable yield reduction (Wang et al., 2006; Warzecha et al., 2011). Since publication of the first study to identify CF parameters from the JIP-test associated with fungal infection in wheat, this is the extension of the method proposed by Ajigboye et al. (2016), applied in barley – F. culmorm pathosystem. In winter wheat the changes in the PSII, as a response to fungal pathogen infection, were quantified from selected parameters resulting from the analysis of the fast fluorescence OJIP transient (Ajigboye et al., 2016). The authors proved that CF parameters were related significantly to known resistance ratings for foliar pathogen (Blmeria graminis) of wheat varieties, pathogen DNA of individual Oculimacula and Fusarium spp. generally existing in stem-base and ear diseases complexes.

The results of our studies showed a varied intensity of disease symptoms both in hulled and hull-less DH lines. Remarkably hulled lines revealed less root susceptibility to infection of F. culmorum expressed in DR and in fresh weight in the plate assay. The findings match results obtained by Warzecha et al. (2012) where less severe symptoms of the infection on leaves were found in hulled oat cultivars when compared to hull-less cultivars. Warzecha et al. (2012) reported that hull-less oat cultivars revealed a 20% higher reduction of leaf weight as compared with hulled cultivars. Similarly, in the case of the hulled genotypes the rating scale evaluation (no visual symptoms of the disease on seedling leaves) as well as seedling leaf weight values may suggest their greater resistance to F. culmorum.

As observed by Warzecha et al. (2015) in the set of barley DH lines the mean values of the seedling root weight were reduced more than twice (2.6 times) as much as the leaf weight, as with the evaluation in DR where the disease symptoms were three times more severe in roots in the group of hulled than in hull-less lines. Other authors showed that the destruction caused by Fusarium seedling blight is much greater in the root system (Grey and Mathre, 1988; Warzecha et al., 2012; Wojciechowski et al., 1997). Also, Ren et al. (2015) has postulated that the symptoms of FSB are predominantly restricted to the root and stem base of seedlings, unlike foliar diseases, since the disease is both seed- or soil-borne.

The root system damage has an impact on physiological processes: uptake and transport of water and mineral salts as well as assimilates distribution, which later affects the development of plants. The results obtained by Ren et al. (2015) indicated that Microdochium nivale and M. majus exhibit preferential pathogenicity towards certain plant tissues. It may also occur in the case of F. culmorum infection since severe damage was associated with roots.

In our studies inoculation in most cases decreased CF parameters, and the reduction was higher in the set of hullless lines comparing to hulled lines. This was most drastically observed in number of reduced active reaction centers (RC/CS) under greenhouse conditions. Under field conditions the most affected by infection parameter was light energy absorption by leaf cross-section (ABS/CS), whereas ETo/CS and RC/CS did not changed significantly. In the present paper the analysis of variance revealed that treatment, genotype, and the interaction of both factors were significant for almost all measured CF parameters (apart from DIo/CS, where the treatment was not significant) in plate assay. Therefore, it was observed that in the population of homozygous DH lines obtained from the F1 generation of two parents differing in their resistance/susceptibility to F. culmorum infection.

Berger et al. (2007) reported reduced CF parameters (Fv/Fm) significantly associated with biotic stress. Also, Ren et al. (2015) reported that infection caused by M. majus significantly reduced the maximum efficiency of PSII in the set of studied wheat cultivars. In our studies this tendency was most visible in the reduced number of active reaction centers in hull-less lines, while in the set of hulled lines this reduction was insignificant. In the field test infection caused not only a reduction of CF parameters, but also yield-related traits. Ajigboye et al. (2016) also observed a significant reduction in PSII efficiency after wheat plants were infected with severe pathogens like F. avenaceum and F. culmorum. The above authors observed a significant decrease of Fv/Fm and active reaction centers on one hand, but an increase of total dissipation of excess excitation energy from PSII reaction centers on the other. Moreover, infection also caused a decrease in electron transport, as was observed by Pinto et al. (2000), who postulated that impairment of photosynthetic efficiency was predominantly caused by the decrease of the mentioned CF parameter.

It is noticeable that the reduction in the number of active reaction centers was greater in hull-less DH lines, while in the set of hulled lines the changes were considerably lower. The above information confirms the observations of other authors that the redox state of PSII can regulate many processes, including the expression of photosynthetic genes and chloroplast biogenesis (Pfannschmidt et al., 2001), leaf colouring during the senescence and anthocyanin biosynthesis in cold (Feild et al., 2001), and also growth rate by changes in hormonal balance (ABA/GAs) (Rapacz, 1998; Rapacz et al., 2003). Based on our results, it can be stated that the redox state of PSII can play an important role in plants’ defense mechanisms. A similar tendency in CF parameters (ABS/CS, DIo/CS and RC/CS were significant, whereas TRo/CS, ETo/CS and RC/CSo were insignificant) was observed in our experiments in plate assay, greenhouse test and field experiment.

If we consider stress caused by infection, the formation of the CF parameter concerning amount of energy dissipated from PSII, estimated as (ABS/CS - TRo/CS) - (DIo/CS), could be interesting. In plate assay this parameter was insignificant but in greenhouse test and field experiment it was significant. In the set of infected hulled lines the amount of energy dissipated from PSII was much higher than in the set of hull-less lines. This could indicate that plants under stress caused by infection can fight with some damage of PSII by higher energy dissipation as suggested by Huner et al. (1993).

In our study inoculation significantly influenced the following CF parameters: ABS/CS, TRo/CS, ETo/CS, RC/CSo, RC/CS in plate assay. All CF parameters were significantly influenced by treatment in greenhouse test and three CF parameters: ABS/CS, DIo/CS, RC/CS in field test. Similar results were reported by Warzecha et al. (2015) who demonstrated highly significant differences between the DH lines and the interaction for the maximum photochemical efficiency (Fv/Fm), and the overall performance index of PSII (PI). Hull-less lines had lower mean PI values than hulled lines for inoculated plants compared to the control plants. Ajigboye et al. (2016), suggest that specific CF parameters that enable the fast detection and differentiation of plant responses may be related to trophic relationship. Necrotrophic pathogens must kill the host tissue to get nutrients (Perfect and Green, 2001). The above authors postulated that wheat response to necrotrophic pathogens like F. avenauceum and F. culmorum were quantified more closely with CF parameters related to PSII efficiency and active PSII RC possibly because of rapid damage associated with aggressive infection. The reduction of photosynthesis efficiency caused by necrotrophic pathogens as presented in previous studies was directly associated with decreasing chlorophyll content in necrotic tissue and decreasing photosynthetic efficiency in green foliar tissue caused by decomposition of cell components, and eliciting enzymes, toxins, and reactive oxygen species from pathogens in order to colonize host tissue (Mengiste, 2012; Warzecha et al., 2015).

In plate assay CF parameters CF parameters had a significant negative correlation with DR (disease rating) of leaves and roots. Higher values of DR (more severe damage of roots and leaves) resulted in lower performance of PSII. So, it provides an extra opportunity to access the level of resistance of various genotypes via an indirect test. In greenhouse, higher values of infected plants FW are connected with better efficiency of PSII. Each of the studied CF parameters could be informative regarding the level of resistance of genotypes.

The impact of infection evaluated under field conditions was clearly visible looking at direct parameters: DR of heads, number of grains per head, weight of grains per head and grain fractions. The reduction of grain size could be associated with the disease impact (or the result of infection enhancing small grain as a disturbance of grain development, storage material shortage and unsettled assimilate transportation). Considering CF parameters the most informative was DIo/CS, which had a significant negative correlation with DR of head and the smallest grain fraction KD1 (< 2.2 mm) and a significant positive correlation with grain fraction KD3 (> 2.5 mm). Therefore, higher values of DIo/CS were related to weaker scab symptoms, as revealed by visual assessment of heads and decreased amount of smallest grain fraction.

The CF parameters were also examined according to their compatibility among the three environments (plate essay for resistance, greenhouse test, field test). It was revealed that more parameters had significant positive correlation in the greenhouse test and field test – ABS/CS, TRo/CS, and RC/CS. Only two parameters (RC/CSo and RC/CS) had a significant positive correlation in the plate assay for resistance and greenhouse test.

Both plate assay and greenhouse test assessed susceptibility to FSB. However, the method of inoculation was different. Therefore, the more relevant method based on CF parameters, which better explains the linkage between FSB and FHB, is inoculating the grain and sowing them in the soil (greenhouse test). The differences in susceptibility assessment to M. majus with various methods of pathogen application was reported by Ren et al. (2015), in which the CF parameters better correlated with FSB or plant trait assessment when comparing the detached leaf inoculation method to soil inoculation.


After infection of barley DH lines by F. culmorum most CF parameters were significantly reduced, and the reduction was higher in the set of hull-less lines compared to hulled lines. The plate assay revealed that the amount of energy used for electron transport (ETo/CS) is negatively correlated with disease rating of leaves and roots and positively with fresh weight of leaves and roots. It provides an extra opportunity to assess the level of resistance of various genotypes via an indirect test.

In the greenhouse test, higher fresh weight of infected plants is connected with better efficiency of PSII based on chlorophyll fluorescence parameters. Each of the studied CF parameters could reveal the resistance levels of genotypes. The field test revealed that the higher DIo/CS values are related to weaker scab symptoms, as revealed by visual assessment of heads and a decreased amount of smallest grain fraction associated with the disease impact. FSB assessed under greenhouse conditions better correlates with FHB under field conditions than plate assay for resistance when considering CF parameters.

Two lines were distinguished according to their performance in laboratory tests, R63N/9 and R63N/4, which possessed the lowest DR, the highest number of grains per ear and the highest values of CF parameters. The lines mentioned above were also least affected by Fusarium head blight.


Mean values ± SE of chlorophyll a fluorescence (CF) parameters and direct parameters (DR – disease rating, FW – fresh weigh of leaves [mg] and yield-related traits) of inoculated and control barley DH lines measured at different tests

Parameter, traitDH linesParent - RK63/1Parent - 1N86

Plate assay

ABS/CS309.9 ± 2.26316.0 ± 1.66310.7 ± 2.71312.9 ± 3.27316.4 ± 5.46306.2 ± 8.73
TRO/CS251.2 ± 1.81256.8 ± 1.22256.3 ± 2.24256.1 ± 2.63256.2 ± 4.10250.8 ± 5.95
ETO/CS111.3 ± 1.53117.2 ± 1.09130.1 ± 2.69118.0 ± 1.74114.5 ± 2.14117.9 ± 1.84
DIO/CS58.8 ± 0.6359.2 ± 0.6154.4 ± 0.9156.8 ± 0.6560.2 ± 1.9555.4 ± 2.78
RC/CSo108.1 ± 1.15117.4 ± 0.80118.4 ± 1.64118.3 ± 0.97112.7 ± 2.33118.9 ± 1.53
RC/CS578.2 ± 7.31634.1 ± 5.32676.9 ± 3.27652.9 ± 5.79598.8 ± 15.31660.3 ± 5.70
DR - leaf23.9 ± 2.090.0 ± 0.07.0 ± 0.940.0 ± 0.058.3 ± 5.210.0 ± 0.0
DR - root67.03 ± 1.283.3 ± 0.4958.7 ± 9.256.3 ± 0.8289.8 ± 3.258.6 ± 0.54
FW - leaf64.1 ± 2.1085.3 ± 2.1170.0 ± 1.5280.0 ± 1.3256.7 ± 4.7490.0 ± 3.28
FW - root24.6 ± 1.2067.7 ± 3.2033.3 ± 5.6790.0 ± 6.1216.7 ± 2.5856.7 ± 4.26

Greenhouse test

ABS/CS270.9 ± 5.00335.6 ± 1.21287.4 ± 5.75333.6 ± 11.92249.4 ± 14.34331.0 ± 10.40
TRO/CS217.8 ± 4.07274.6 ± 0.97233.9 ± 4.40273.2 ± 9.80199.1 ± 12.04270.4 ± 8.70
ETO/CS107.7 ± 2.54146.0 ± 0.76117.4 ± 4.45145.3 ± 6.2797.7 ± 7.17143.2 ± 6.19
DIO/CS53.4 ± 1.1961.0 ± 0.2953.5 ± 1.3560.4 ± 2.2250.3 ± 3.7360.6 ± 1.72
RC/CSo96.7 ± 2.24131.6 ± 0.82102.5 ± 5.35129.6 ± 6.2184.3 ± 6.92131.5 ± 8.44
RC/CS501.4 ± 12.78725.5 ± 4.86551.0 ± 26.12716.0 ± 35.03421.8 ± 46.21719.1 ± 48.43
DR - leaf58.1 ± 2.463.3 ± 1.1533.1 ± 4.686.3 ± 2.0880.7 ± 5.208.6 ± 4.03
FW - leaf139.0 ± 4.78246.7 ± 3.89126.7 ± 5.02203.3 ± 8.2660.0 ± 3.12183.3 ± 10.30

Field test

ABS/CS599.3 ± 6.65666.6 ± 9.51622.3 ± 66.67704.3 ± 12.69625.5 ± 34.82658.2 ± 9.58
TRO/CS470.6 ± 5.47499.3 ± 7.19485.0 ± 69.31534.5 ± 4.95502.0 ± 22.01523.2 ± 5.98
ETO/CS194.9 ± 4.05191.2 ± 4.65209.2 ± 43.10206.7 ± 15.16232.6 ± 11.12215.4 ± 5.00
DIO/CS128.8 ± 2.90167.3 ± 7.46137.2 ± 23.77169.8 ± 8.65123.5 ± 15.06135.0 ± 4.28
RC/CSo168.2 ± 2.77171.7 ± 3.04171.1 ± 29.84177.0 ± 10.04196.0 ± 6.51180.7 ± 4.96
RC/CS845.3 ± 19.66781.8 ± 24.39839.7 ± 202.6808.5 ± 93.251022.1 ± 95.26900.6 ± 34.74
DR - head61.3 ± 3.24-48.2 ± 2.98-64.0 ± 5.12-
KNS14.4 ± 2.9519.8 ± 2.0116.2 ± 1.9619.6 ± 1.0221.5 ± 1.1523.9 ± 0.98
KWS0.43 ± 0.120.88 ± 0.100.48 ± 0.120.98 ± 0.130.44 ± 0.160.95 ± 0.09
KD128.2 ± 12.5772.6 ± 9.2428.6 ± 10.2360.3 ± 11.2549.1 ± 14.274.4 ± 12.8
KD234.5 ± 9.7718.9 ± 7.5639.3 ± 5.2333.0 ± 6.3136.9 ± 7.1218.4 ± 2.35
KD337.3 ± 12.148.6 ± 2.4132.0 ± 6.326.6 ± 1.2114.0 ± 2.517.2 ± 1.12

KWS – kernel weight per spike, KNS – number of kernels per spike, KD1, KD2 and KD3 – kernel diameter: > 2.5 mm. 2.5-2.2 mm and < 2.2 mm, respectively

F-statistic from analysis of variance for chlorophyll a fluorescence (CF) parameters and direct parameters (DR – disease rating, FW – fresh weigh) of inoculated and control barley DH lines measured at different tests

CF parametersPlate assayGreenhouse testField test

T (df=1)G (df=31)G × T (df=31)T (df=1)G (df=31)G × T (df=31)T (df=1)G (df=31)G × T (df=31)

DR – leaf-24.35**-355.12**15.31**17.03**---
FW – leaf51.83**1.73*0.62201.42**3.91**1.70*---

DR – Root7148.52**7.02**9.11**------
FW – Root233.51**3.67**1.05------
DR – head------0.92

*P < 0.05;

**P < 0.01

T – treatment, G – genotype, T × G – treatment × genotype interaction KWS – kernel weight per spike, KNS – number of kernels per spike, KD1, KD2 and KD3 – kernel diameter: > 2.5 mm. 2.5-2.2 mm and < 2.2 mm, respectively

Orthogonal contrasts for chlorophyll a fluorescence (CF) parameters between hulled and hull-less barley DH lines at plate assay, greenhouse and field tests

CF parametersPlate assayGreenhouse testField test


*P < 0.05;

**P < 0.01

Correlation coefficients between chlorophyll a fluorescence (CF) parameters and disease rating (DR) and fresh weight of leaves and roots in plate assay

CF parametersTreatmentDR - leafDR - rootFresh weight - leafFresh weight - root


*P < 0.05;

**P < 0.01

1– in control disease symptoms on leaves was only sporadically observed;

Correlation coefficients between chlorophyll a fluorescence (CF) parameters and disease rating (DR) and fresh weight of leaves revealed in greenhouse test

CF parametersTreatmentDR - leafFresh weight - leaf


*P < 0.05;

**P < 0.01

Correlation coefficients between chlorophyll a fluorescence (CF) parameters and disease rating of heads (DR), number of grains per head (KNS), weight of grains per head (KWS) and kernel diameter: KD1, KD2 and KD3 revealed under field test

CF parameterTreatmentDRKNSKWSKD1KD2KD3


*P < 0.05;

**P < 0.01

KD1, KD2 and KD3 – kernel diameter: > 2.5 mm. 2.5-2.2 mm and < 2.2 mm, respectively

Correlation coefficients between chlorophyll a fluorescence (CF) parameters measured under plate assay, greenhouse and field tests

TreatmentCF parameters

plate assay – greenhouse test


plate assay – field test


greenhouse test – field test


*P < 0.05;

**P < 0.01

  1. Adamski T, Chełkowski J, Goliński P, Kaczmarek Z, Kostecki M, Perkowski J, Surma M, and Wiśniewska H. 1999. Yield reduction and mycotoxin accumulation in barley doubled haploids inoculated with Fusarium culmorum (W.G.Sm.) Sacc. J Appl Genet 40: 73-84.
  2. Ajigboye OO, Murchie EH, and Ray RV. 2014. Foliar application of isopyrazam and epoxiconazole improves photosystem II efficiency, biomass and yield in winter wheat. Pestic Biochem Physiol 114: 52-60.
    Pubmed CrossRef
  3. Ajigboye OO, Bousquet L, Murchie EH, and Ray RV. 2016. Chlorophyll fluorescence parameters allow the rapid detection and differentiation of plant responses in three different wheat pathosystems. Funct Plant Biol 43: 356-369.
  4. Arseniuk E, Góral T, and Czembor HJ. 1993. Reaction of triticale, wheat and rye accessions to graminaceous Fusarium spp. infection at the seedling and adult plant growth stages. Euphytica 70: 175-183.
  5. Arseniuk E, Foremska E, Góral T, and Chełkowski J. 1999. Fusarium head blight reactions and accumulation of deoxynivalenol (DON) and some of its derivatives in kernels of wheat. triticale and rye. J Phytopathol 147: 577-590.
  6. Baker NR, and Rosenqvist E. 2004. Applications of chlorophyll fluorescence can improve crop production strategies: an examination of future possibilities. J Exp Bot 5: 1607-1621.
    Pubmed CrossRef
  7. Bauriegel E, Giebel A, and Herppich WB. 2010. Rapid Fusarium head blight detection on winter wheat ears using chlorophyll fluorescence imaging. J Appl Bot Food Qual 83: 196-203.
  8. Bolhar-Nordenkampf HR, and Öquist G. 1993. Chlorophyll fluorescence as a tool in photosynthesis research. In: Photosynthesis and production in a changing environment: a field and laboratory manual, eds. by DO. Hall, JMO. Scurlock, HR. Bolhàr-Nordenkampf, RC. Leegood, and SP. Long , pp. 193-206. Springer, Dordrecht, The Netherlands.
  9. Bottalico A, and Perrone G. 2002. Toxigenic Fusarium species and mycotoxins associated with head blight in small – grain cereals in Europe. Eur J Plant Pathol 108: 611-624.
  10. Buerstmayr H, Ban T, and Anderson JA. 2009. QTL mapping and marker-assisted selection for Fusarium head blight resistance in wheat: a review. Plant Breed 128: 1-26.
  11. Chełkowski J, and Mańka M. 1983. The ability of Fusaria pathogenic to wheat, barley and corn to produce zearalenone. J Phytopathol 106: 354-359.
  12. Chełkowski J, Kaptur P, Tomkowiak M, Kostecki M, Goliński P, Ponitka A, Sacute;lusarkiewicz-Jarzina A, and Bocianowski J. 2000. Moniliformin accumulation in kernels of triticale accessions inoculated with Fusarium avenaceum in Poland. J Phytopathol 148: 433-449.
  13. Cowger C, Patton-Ozkurt J, Brown-Guedira G, and Perugini L. 2009. Post-anthesis moisture increased Fusarium head blight and deoxynivalenol levels in North Carolina winter wheat. Phytopathology 99: 320-327.
    Pubmed CrossRef
  14. Czyczyło-Mysza I, Tyrka M, Marcińska I, Skrzypek E, Karbarz M, Dziurka M, Hura T, Dziurka K, and Quarrie SA. 2013. Quantitative trait loci for leaf chlorophyll fluorescence parameters. chlorophyll and carotenoid contents in relation to biomass and yield in bread wheat and their chromosome deletion bin assignments. Mol Breed 32: 189-210.
    Pubmed KoreaMed CrossRef
  15. Demetriou G, Neonaki C, Navakoudis E, and Kotzabasis K. 2007. Salt stress impact on the molecular structure and function of the photosynthetic apparatus: the protective role of polyamines. Biochim Biophys Acta 1767: 272-280.
    Pubmed CrossRef
  16. Desjardins AE. 2006. Fusarium mycotoxins. Chemistry, genetics and biology . APS Press, St. Paul, MN, USA. 260 pp.
  17. Foroud NA, and Eudes F. 2009. Trichothecenes in cereal grains. Int J Mol Sci 10: 147-173.
    Pubmed KoreaMed CrossRef
  18. Fracheboud Y, and Leipner J. 2003. The application of chlorophyll fluorescence to study light, temperature and drought stress. In: Practical applications of chlorophyll fluorescence in plant biology, eds. by JR. DeEll, and PMA. Tiovonen , pp. 125-150. Springer, Boston, MA, USA.
  19. Gorbe E, and Calatayud A. 2012. Applications of chlorophyll fluorescence imaging technique in horticultural research: a review. Sci Hortic 138: 24-35.
  20. Grey W, and Mathre DE. 1988. Evaluation of spring barley for reaction to Fusarium seedling blight and root rot. Can J Plant Sci 68: 23-30.
  21. Huner NP, Öquist G, Hurry VM, Krol M, Falk S, and Griffith M. 1993. Photosynthesis, photoinhibition and low temperature acclimation in cold tolerant plants. Photosynth Res 37: 19-39.
    Pubmed CrossRef
  22. Imathiu SM, Hare MC, Ray RV, Back M, and Edwards SG. 2010. Evaluation of pathogenicity and aggressiveness of F. langsethiae on oat and wheat seedlings relative to known seedling blight pathogens. Eur J Plant Pathol 126: 203-216.
  23. Inch SA, and Gilbert J. 2003. Survival of Gibberella zeae in Fusarium–Damaged wheat kernels. Plant Dis 83: 282-287.
    Pubmed CrossRef
  24. Kasha KJ, and Kao KN. 1970. High frequency haploid production in barley (Hordeum vulgare L.). Nature 225: 874-876.
    Pubmed CrossRef
  25. Ma HX, Ge HJ, Zhang X, Lu WZ, Yu DZ, Chen H, and Chen JM. 2009. Resistance to Fusarium head blight and deoxynivalenol accumulation in Chinese barley. J Phytopathol 157: 166-171.
  26. Magan N, Hope R, Colleate A, and Baxter ES. 2002. Relationship between growth and mycotoxin production by Fusarium species. biocides and environment. Eur J Plant Pathol 108: 685-690.
  27. Mardi M, Pazouki L, Delavar H, Kazemi MB, Ghareyazie B, Steiner B, Nolz R, Lemmens M, and Buerstmayr H. 2006. QTL analysis of resistance to Fusarium head blight in wheat using a ‘Frontana’- derived population. Plant Breed 125: 313-317.
  28. Marin S, Ramos AJ, Cano-Sancho G, and Sanchis V. 2013. Mycotoxins: occurrence, toxicology. and exposure assessment. Food Chem Toxicol 60: 218-237.
    Pubmed CrossRef
  29. Maxwell K, and Johnson GN. 2000. Chlorophyll fluorescence – a practical guide. J Exp Bot 51: 659-668.
    Pubmed CrossRef
  30. Mengiste T. 2012. Plant immunity to necrotrophs. Annu Rev Phytopathol 50: 267-294.
    Pubmed CrossRef
  31. Mesterházy A. 1995. Types and components of resistance to Fusarium head blight of wheat. Plant Breed 114: 377-386.
  32. Mesterházy A. 2002. Role of deoxynivalenol in aggressiveness of Fusarium graminearum and F. culmorum and in resistance to Fusarium head blight. Eur J Plant Pathol 108: 675-684.
  33. Mesterházy A, Bartók T, Mirocha CG, and Komoróczy R. 1999. Nature of wheat resistance to Fusarium head blight and the role of deoxynivalenol for breeding. Plant Breed 118: 97-110.
  34. Miedaner T. 1997. Breeding wheat and rye for resistance to Fusarium diseases. Plant Breed 116: 201-220.
  35. Miedaner T, Reinbrecht C, Lauber U, Schollenberger M, and Geiger HH. 2001. Effects of genotype and genotype x environment interaction on deoxynivalenol accumulation and resistance to Fusarium head blight in rye, triticale, and wheat. Plant Breed 120: 97-105.
  36. Nielsen LK, Jensen JD, Nielson GC, Spliid NH, Thomsen IK, Justesen AF, Collinge DB, and Jørgensen LN. 2011. Fusarium head blight of cereals in Denmark: species complex and related mycotoxins. Phytopathology 101: 960-969.
    Pubmed CrossRef
  37. Nielsen LK, Justesen AF, Jensen JD, and Jørgensen LN. 2013. Microdochium nivale and Microdochium majus in seed samples of Danish small grain cereals. Crop Prot 43: 192-200.
  38. Nielsen LK, Cook DJ, Edwards SG, and Ray RV. 2014. The prevalence and impact of Fusarium head blight pathogens and mycotoxins on malting barley quality in UK. Int J Food Microbiol 179: 38-49.
    Pubmed KoreaMed CrossRef
  39. O’Neill PM, Shanahan JF, and Schepers JS. 2006. Use of chlorophyll fluorescence assessments to differentiate corn hybrid response to variable water conditions. Crop Sci 46: 681-687.
  40. Pereira WE, de Siqueira DL, Martínez CA, and Puiatti M. 2000. Gas exchange and chlorophyll fluorescence in four citrus rootstocks under aluminium stress. J Plant Physiol 157: 513-520.
  41. Perfect SE, and Green JR. 2001. Infection structures of biotrophic and hemibiotrophic fungal plant pathogens. Mol Plant Pathol 2: 101-108.
    Pubmed CrossRef
  42. Pfannschmidt T, Allen JF, and Oelmüller R. 2001. Principles of redox control in photosynthesis gene expression. Physiol Plant 112: 1-9.
  43. Pickering RA, and Devaux P. 1992. Haploid production: Approaches and use in plant breeding. In: Barley: Genetics Biochemistry, molecular biology and biotechnology, ed. by PR. Shewry , pp. 519-547. CAB International, Wallingford, UK.
  44. Pinto LSRC, Azevedo JL, Pereira JO, Vieira MLC, and Labate CA. 2000. Symptomless infection of banana and maize by endophytic fungi impairs photosynthetic efficiency. New Phytol 147: 609-615.
  45. Rapacz M. 1998. The after-effects of temperature and irradiance during early growth of winter oilseed rape (Brassica napus L var oleifera cv Gorczanski) seedlings on the progress of their cold acclimation. Acta Physiol Plant 20: 73-78.
  46. Rapacz M, Waligórski P, and Janowiak F. 2003. ABA and gibberellin-like substances during prehardening, cold acclimation, de- and reacclimation of oilseed rape. Acta Physiol Plant 25: 151-161.
  47. Ren R, Yang X, and Ray RV. 2015. Comparative aggressiveness of Microdochium nivale and M. majus and evaluation of screening methods for Fusarium seedling blight resistance in wheat cultivars. Eur J Plant Pathol 141: 281-294.
  48. Rolfe SA, and Scholes JD. 2010. Chlorophyll fluorescence imaging of plant pathogen interactions. Protoplasma 247: 163-175.
    Pubmed CrossRef
  49. Schroeder HW, and Christiansen JJ. 1963. Factors affecting resistance of wheat to scab caused by Gibberella zeae. Phytopathology 53: 831-838.
  50. Smillie RM, and Nott R. 1982. Salt tolerance in crop plants monitored by chlorophyll fluorescence in vivo. Plant Physiol 70: 1049-1054.
    Pubmed KoreaMed CrossRef
  51. Snijders CH. 2004. Resistance in wheat to Fusarium infection and trichothecene formation. Toxicol Lett 153: 37-46.
    Pubmed CrossRef
  52. Strasser BJ, and Strasser RJ. 1995. Measuring fast fluorescence transients to address environmental questions: the JIP-Test. In: Photosynthesis: from light to biosphere, ed. by P. Mathis , pp. 977-980. KAP Press, Dordrecht, The Netherlands.
  53. Strasser RJ, and Tsimilli-Michael M. 1998. Activity and heterogeneity of PS II probed in vivo by the chlorophyll-a fluorescence rise O-(K)-J-I-P. In: Photosynthesis: mechanisms and effects, ed. by G. Garab , pp. 4321-4324. KAP Press, Dordrecht, The Netherlands.
  54. Strasser RJ, Srivastava A, and Tsimilli-Michael M. 2000. The fluorescence transient as a tool to characterize and screen photosynthetic samples. In: Probing photosynthesis: mechanisms, regulation and adaptation, eds. by M. Yunus, U. Pathre, and P. Mohanty , pp. 445-483. Taylor and Francis, London, UK.
  55. Wang H, Hwang SF, Eudes F, Chang KF, Howard RJ, and Turnbull GD. 2006. Trichothecenes and aggressiveness of Fusarium graminearum causing seedling blight and root rot in cereals. Plant Pathol 55: 224-230.
  56. Warzecha T, Adamski T, Kaczmarek Z, Surma M, Goliński P, Perkowski J, Chełkowski J, Wiśniewska H, Krystkowiak K, and Kuczyńska A. 2010. Susceptibility of hulled and hulless barley doubled haploids to Fusarium head blight. Cereal Res Commun 38: 220-232.
  57. Warzecha T, Adamski T, Kaczmarek Z, Surma M, Chełkowski J, Wiśniewska H, Krystkowiak K, and Kuczyńska A. 2011. Genotype–by-Environment interaction of barley DH lines infected with Fusarium culmorum (W.G.Sm.) Sacc. Field Crops Res 120: 21-30.
  58. Warzecha T, Zieliński A, Skrzypek E, Wójtowicz T, and Moś M. 2012. Effect of mechanical damage on vigor. physiological parameters. and susceptibility of oat (Avena sativa) to Fusarium culmorum infection. Phytoparasitica 40: 29-36.
  59. Warzecha T, Skrzypek E, and Sutkowska A. 2015. Effect of Fusarium culmorum infection on the selected physiological and biochemical parameters of barley (Hordeum vulgare L.) DH lines. Physiol Mol Plant Pathol 89: 62-69.
  60. Wiśniewska H, Stępień Ł, Waśkiewicz A, Beszterda M, Góral T, and Belter J. 2014. Toxigenic Fusarium species infecting wheat heads in 2009 in selected regions of Poland. Central Eur J Biol 9: 163-172.
  61. Wojciechowski S, Chełkowski J, Ponitka A, and Sacute;lusarkiewicz-Jarzina A. 1997. Evaluation of spring and winter wheat reaction to Fusarium culmorum and Fusarium avenaceum. J Phytophatol 145: 99-103.
  62. Yang ZP, Gilbert J, Fedak G, and Somers DJ. 2005. Genetic characterization of QTL associated with resistance to Fusarium head blight in a doubled-haploid spring wheat population. Genome 48: 187-196.
    Pubmed CrossRef
  63. Živcák M, Brestic M, Olšovská K, and Slamka P. 2008. Performance index as a sensitive indicator of water stress in Triticum aestivum L. Plant Soil Environ 54: 133-139.

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