Cite this asLebon G, Rondeau M, Sanchez L, Ait Barka E, Vaillant-Gaveau N, et al. (2016) Modulation of the Activity of Enzymes Involved in Carbohydrate Metabolism during Flower Development of Grapevine (Vitis Vinifera L.). Open J Plant Sci 1(1): 010-017, DOI: 10.17352/ojps.000003
In order to further understand the relationships between flower development and sugar metabolism in grapevine, the fluctuations of both starch and sucrose contents were compared with the activity of their related enzymes, in the inflorescences, from the appearance of flower buds until the fruit set. The measurements were carried out on GW and PN cvs., differing in their sensitivity to the flower abscission. The meiosis stage, which is a crucial step for the achievement of sexual reproduction, was particularly screened. Results indicate that the main differences in carbohydrate metabolism occur during meiosis. In the inflorescences of both cvs., variations of enzyme activities can be correlated with their differences in sugar contents. Starch fluctuations were mediated by the activity of amylases (alpha- and beta-) rather than by starch synthase. Changes of sucrose were correlated with the activity of Starch Synthase degradation, both cytoplasmic and wall-bounded invertases but not with the Sucrose Phosphate Synthase activity. Finally, the significant increase of sucrose degrading enzyme activities, such as Starch Synthase degradation, cytoplasmic invertase, and wall-bound invertase, observed after the flower separating stage was interpreted as the first sign of the strong physiological modifications occurred in the ovaries between fertilization and the fruit formation.
Grapevine (Vitis Vinifera L.) is naturally affected by the flower abscission depending on both physiological factors such as the carbon nutrition  and cultivars , and environmental factors  such as chilling or heat [4-7]. Under optimal growth conditions, the intensity of flower drop represents a specific trait of each cultivar (cv.). For instance, in the Gewurztraminer (GW) cv., flower drop corresponds to 18 % of the total flowers whereas in the Pinot noir (PN) cv., the abscission of flowers reaches 35 % [1,8]. However, when environmental stress occurs, the rate of flower abscission may change dramatically, reaching up to 80% in the GW cv. . In this respect, the various cultivars (cvs.) of grapevine can be classified into two types according to their sensitivity to the flower drop under stressing conditions: (i) sensitive cvs. Such as GW, and (ii) non-sensitive cvs. Such as PN.
Under optimal growth conditions, the rate of flower abscission is correlated with the pathway of both male and female organ development and to the amount of carbohydrates in the inflorescences [3,9]. Comparing GW and PN, it was shown that the development of reproductive structures in PN is earlier than in GW . Moreover, gametophyte development is dependent on sugar physiology, and any perturbation in carbohydrate metabolism during flower development induces the gametophyte abortion [10,11], leading to reduce the success of fertilization [12,13]. In particular, the reproductive organs are sensitive to modifications of carbohydrate physiology when fertile tissues reach meiosis . At this key step, the rate of fertilization depends on the cultivars and can be correlated to the carbohydrate status of grapevine inflorescence .
The pathway of sugar fluctuations in woody plant organs is the result of complex regulation processes involving photosynthesis [14-16] and reserve mobilization/restoration [17,18]. Carbon assimilated in photosynthetic leaves is translocated as sucrose to sink organs, where it is converted into glucose and fructose or stored as starch reserves. Most often, the control of carbohydrate variations is reliable with feedback regulation of photosynthesis by carbon metabolites [19,20], affecting the related enzyme activities [21-23]. In the developing inflorescence of grapevine, it was shown that carbohydrates are supplied by reserve mobilization from perennial organs  and by photosynthesis in both leaves  and inflorescences [25-27].
Starch is of great importance as sugar nutrient reserve in the developing flowers [28,29]. Starch-degrading enzymes in plant tissues include two kinds of amylases . The alpha-amylase [αA - EC 18.104.22.168] is an endo-enzyme cutting randomly amylose and amylopectin chains into dextrins . In parallel, the beta-amylase [βA A - EC 22.214.171.124] is an exo-enzyme that releases molecules of maltose from amylose chains . These two enzymes reflect distinct modes of starch mobilization and may represent a potential marker among the various cultivars. Other enzymes involved in starch biosynthesis are starch synthase [StSy - EC 126.96.36.199], which synthetises amylose by reaction with ADPGlc and starch branching enzyme [EC 188.8.131.52] for the synthesis of amylopectin by reacting with the amylose chains [33,34].
The inflorescence is the plant organ containing the highest concentration of soluble sugars during its development and sucrose represents the main form of circulating sugar [35,36], namely in young grapevine inflorescences at key developmental steps . Three enzymes are directly involved in sucrose metabolism : (i) the sucrose phosphate synthase [SPS - EC 184.108.40.206], which plays a major role in sucrose biosynthesis ; (ii) the sucrose synthase [SS - EC 220.127.116.11] that catalyses the reversible conversion of sucrose and UDP into fructose and UDP-glucose [22,38]; and (iii) the invertase [Inv - EC 18.104.22.168], which is an hydrolase, cleaving sucrose irreversibly into glucose and fructose [22,38]. Several Inv isoforms either cytoplasmic (Cy Inv) or wall-bounded (WB Inv) have been described in flower organs , pointing different sucrose utilization pathways as well. In addition to these three enzymes, SS is also considered to assume a sucrose synthesis in some plant tissues .
In order to further understand the relationships between flower development and sugar metabolism in grapevine, we assayed related-enzymes activity in the inflorescences accurately from the appearance of flower buds until the fruit set. In this aim, we used the GW and the PN cvs., differing in their sensitivity to flower abscission. We focused on the meiosis step, which was shown to be a crucial point for the achievement of sexual plant reproduction and reflecting major differences in sugar physiology in the two cultivars [1,41]. Further, we particularly focused on the enzymes involved in the synthesis and degradation of both starch and sucrose since they are the major sugars in the inflorescences of grapevine during the flower development .
Thirty-year-old field-grown grapevines (Vitis Vinifera L.) GW (flower abscission sensitive) cv. (clone 47) and PN (non-sensitive) cv. (clone 162) were grown in Bergheim (France) following similar cultural practices. Development stages were identified according to the BBCH (Biologische Bundesanstalt, Bundessortenamt and CHemical industry) scale . Inflorescences were investigated during their whole development, from the “visible cluster” stage (BBCH53) up to fruit set (BBCH71). For further precision, especially at the key step meiosis, 2 additional stages were added between the “separated cluster” stage (BBCH55) and the “separated floral buds” stage (BBCH57): 2 and 8 days after BBCH55 corresponding to female meiosis in PN and GW respectively . Inflorescences were collected at the same hour during the day to avoid circadian fluctuations according to eight development stages (DS) as follows:
Inflorescences were collected at each DS, frozen in liquid N2 and stored at -80°Cuntil sugar or enzyme extraction and activity determination.
Lyophilized inflorescences were ground in a mortar with Fontainebleau sand and 10 volumes of ethanol 80°. Sugars were then extracted for 15 min at 84°C under continual agitation. After adjusting the volume to 5 mL with distilled water, the extract was centrifuged at 4°C for 10 min at 11,000g. The supernatant was used for soluble sugar determination. For starch, the pellet previously obtained was suspended in a mixture containing dimethylsulfoxide: hydrochloric acid 8N (8:2) and starch was dissolved during 30 min at 60°C under continual agitation. After cooling, the extract was centrifuged at 20 °C for 10 min at 13,000g and the supernatant was kept at -80°C until use.
Sucrose was hydrolyzed to D-glucose and D-fructose in the presence of a β-fructosidase. D-glucose was phosphorylated and oxidized in the presence of NADP to gluconate-6-phosphate and NADPH, H+. The amount of NADPH, H+ formed was determined by means of its absorbance at 340 nm. D-glucose formed was then determined as described above and compared with a blank without β-fructosidase.
Aliquots of 100 µL of the extract were used to determine starch concentration. The aliquot was mixed with 100 µL of Lugol iodine solution (38.3 mM KI and 2.8 mM I2 in 0.25 M HCl). After 15 min, the absorbance was read spectrophotometrically at 620 nm. A blank was performed with the starch solvent (DMSO: HCl, 8:2) instead of the extract. Preparation of enzyme extract each protocol was performed at 0-4°C according to modified procedures from Nakamura and Yuki . The inflorescences were ground and 500 mg were homogenized with 5 mL of chilled buffer containing 100 mM Tris-Hcl (pH 6.5), 8 mM MgCl2, 2 mM EDTA, 1 mM DTT and 0.1 mM PMSF. The homogenate was transferred to Eppendorf tubes and centrifuged for 5 min at 14,000g at 4°C. The supernatant was collected, stored at -80°C and used as enzyme source. The pellet was washed twice, suspended with the grinding solution and used for the assay of wall-bound invertase. Protein concentration in each sample was determined using a Bio-Rad DC protein assay kit (Bio-Rad, Hercules, CA, USA) and BSA as standard.
Assays were carried out in the range of enzyme concentrations where the activity increased linearly with time and substrate concentration.
Starch synthase (StSy - EC 22.214.171.124) - The assay was conducted according to the modified protocol of Nakamura et al. . An aliquot of 50 µL of the enzyme extract was mixed to 230 µL of 1.6 mM ADP-glucose, 0.7 mg amylopectin and 15 mM DTT preparing in 50 mM HEPES-NaOH at pH 7.4. After 20 min of incubation at 30°C, the enzyme was inactivated by placing the mixture in a boiling-water bath for 30 sec. Then 100 µL of a 50 mM HEPES-NaOH pH 7.4 buffer, containing 4 mM PEP, 200 mM KCl, 10 mM MgCl2, and pyruvate kinase (1.2 unit) were added and the reaction mixture was incubated for 30 min at 30°C. The ADP produced by the starch synthase reaction was converted to ATP and the resulting solution was heated in a boiling-water bath for 30 sec and then subjected to centrifugation for 5 min at 10,000g. The supernatant (300 µL) was mixed to 300 µL of 50 mM HEPES-NaOH (pH 7.4), 10 mM glucose, 20 mM MgCl2, and 2 mM NADP. The starch synthase activity was determined as the increase of absorbance at 340 nm after the addition of 1 µL each of hexokinase (1.4 units) and G6P dehydrogenase (0.35 unit). Data were displayed in µg formed starch per mg of proteins per hour.
Alpha amylase (αA - EC 126.96.36.199) - To estimate this activity, the α-amylase enzyme was first inactivated by heating 1 mL of enzyme source for 15 min at 70°C . After centrifugation at 10,000g for 15 min, 100 µL of supernatant were added to 200 µL of substrate (0.15% starch, 20 mM CaCl2, and 50 mM NaCl prepared in 50 mM sodium acetate buffer at pH 4.8). The mixture was incubated for 60 min at 37°C and the reaction stopped by addition of 800 µL of an iodine solution (38.3 mM KI and 2.8 mM I2 in 0.25 M HCl) and 3.2 mL of dH2O. The residual starch content was then determined spectrophotometrically at 620 nm. Data were expressed in µg of hydrolyzed starch per mg of proteins per hour.
Beta amylase (βA - EC 188.8.131.52) - Estimation of the β-amylase activity was performed at pH 3.6 in order to inhibit the β-amylase . An aliquot of 200 µL of the enzyme extract was incubated for 60 min at 20°C in 200 µL of 1% starch and 0.78 mM ethylenediaminetetraacetic acid (EDTA) prepared in 50 mM sodium citrate buffer (pH 3.6). The reaction was stopped by adding 400 µL of a revelation solution (43.8 mM 3,5-dinitrosalicyclic acid, 0.4 M NaOH, and 1.06 M sodium/potassium tartrate). Samples were incubated for 5 min at 95°C, and the absorbance measured at 540 nm. Data were displayed in µg of formed maltose per mg of proteins per hour.
Sucrose Synthase (SSs - EC 184.108.40.206) and Sucrose Phosphate Synthase (SPS - EC 220.127.116.11). The SSs and SPS activities were determined according to Kubo et al. (2001). An aliquot of 100 µL of enzyme extract was mixed to 50 µL of 0.05 M Tris-HCl (pH 7.5) containing 100 mM UDP-glucose, 100 mM fructose and 10 mM MgCl2. The assay was conducted for 30 min at 25°C and terminated by adding 150 µL of 1 N NaOH. A blank was prepared by adding 1 N NaOH immediately after the onset of the assay. Afterwards, unreacted hexoses in the reaction mixture were destroyed by heating for 10 min at 100°C. To determine the amount of synthesized sucrose, 3 mL of 0.15% anthrone in 13.7 M H2SO4 were added and the mixture was incubated for 20 min at 40°C. The SS activity was calculated as the increase of absorbance at 620 nm, and the data were expressed in µg of formed sucrose per mg of proteins per hour. SPS was assayed following the same protocol than SS, except that fructose was replaced to fructose-6-phosphate.
Sucrose Synthase (SSd - EC 18.104.22.168) - The SS cleavage activity was measured according to Kubo et al. . An aliquot 200 µL of enzyme source was mixed to 50 µL of 0.05 M Tris-HCl (pH 7.5) containing 50 mM sucrose. The reaction was performed for 30 min at 25°C and terminated by adding 250 µL of 1 N NaOH. A blank was prepared by adding 1N NaOH at the onset of the assay. Afterwards, hexoses were destroyed by heating for 10 min at 100°C and an aliquot (50 µL) was used for sucrose determination using the anthrone method described above. The SSd activity was measured as the decrease in absorbance of 620 nm and expressed in µg of degraded sucrose per mg of proteins per hour.
Acid invertase (EC 22.214.171.124) - Wall-bound and soluble acid invertase activities were measured according to the modified protocol of Dreier et al. . The pellet of the enzyme extract was used for wall-bound invertase (WB Inv), whereas the supernatant was used for determining the cytosolic invertase (Cy Inv) activity. An aliquot of 100 µL was mixed to 400 µL with 0.2 M acetate buffer (pH 4.0). The reaction was started by adding 800 µL of 0.225 M sucrose, extended for 30 min at 30°C and was stopped by adding 1 mL of DNSA-reagent (3,5-dinitrosalicylic acid 1%), in 0.5 M KOH and 1 M K/Na-tartrate. Glucose (0.5 µmol) was supplied to avoid oxygen interference at low reducing sugar concentrations and the mixture was boiled for 10 min. After cooling, the invertase activity was calculated as the mean of absorbance at 560 nm and expressed in µg formed glucose per mg of proteins per hour. The vacuolar invertase activity was not assayed because not involved in the carbon metabolism of both male and female reproductive structures [10,50].
For each stage of flower development, 5 assays were performed from five inflorescences of five different plants, and three independent readings were carried out. Each result was the mean ± SE of these data. Mean comparison was carried out using Student’s t-test, and difference was considered as significant at the P = 0.05 level.
Globally starch fluctuated similarly in the GW and the PN inflorescences, with a global decrease during the flower development. Nevertheless, some remarkable differences can be noticed, especially from DS2 to DS4, and at DS7 (Figure 1a). During the period of both male and female meiosis (DS2 to DS4), starch level decreased in both cvs., but remained higher (around 2 fold at DS3) in GW than in PN until DS4 (5.0 ± 0.4 % DW in GW and 3.9 ± 0.3 % DW in PN). Afterwards, a wave of amylogenesis/amylolysis was detected in the inflorescences of both cvs. With a higher amount of starch in GW (6.2 ± 0.5 % DW in GW and 4.3 ± 0.2 % DW in PN) at flower bloom (DS7). Sucrose content fluctuated irregularly during the flower development in the two cvs. (Figure 1b). The sucrose content was relatively weak during the whole development in the two cvs. (Less than 4% DW), sometimes closed to 0% of dry weight (DS2 and DS3 in PN or DS5 in GW). Nevertheless, at DS3, inflorescences exhibited a peak of sucrose in PN (7.1 ± 4.1 % DW) and GW (16.6 ± 1.1 % DW). The sucrose level decreased afterwards, then remained low until the fruit set.
The rate of starch synthesis in inflorescences was evaluated by assaying StSy activity during the flower development (Figure 2a). In both GW and PN cvs., the StSy activity was in a range of 0.085 µg formed amylose.mg protein-1.h-1 at DS1, then decreased by 70% at DS2. Afterwards, the pattern of activity varied according to the cv. Thus, in GW, the activity fluctuated in accordance with the starch degradation, remained around 0.02 µg formed amylose.mg protein-1.h-1 until DS4, then increased to reach a peak at DS6 (0.08 µg formed amylose.mg protein-1.h-1) followed by a slight decrease (0.06 µg formed amylose.mg protein-1.h-1 at DS8). In PN, the variation of StSy activity also corresponded to starch fluctuations in the inflorescence (Figure 1a). The activity increased up to 0.07 µg formed amylose.mg protein-1.h-1 at DS4, and remained stable until the fruit set (Figure 2a).
Both amylases displayed noticeable differences between the two cvs. In term of fluctuations during the flower development (Figure 2b,c) but correlated well with variations measured in starch degradation/synthesis (Figure 1a). In GW, the αA activity globally coincided with starch variations (Figure 2b). The highest was reached at DS1 and DS2, ranging 0.21 µg of hydrolysed starch.mg protein-1.h-1. The level transitory fell to 0.05 µg of hydrolysed starch.mg protein-1.h-1 at DS3. Then, a new peak of the enzyme activity was registered during DS4 and DS5. Finally, the αA activity decreased until being detectable during the two last developmental stages. In PN, the αA activity poorly fluctuated as the starch content in inflorescences. It was ranging approximately 0.1 µg of hydrolyzed starch.mg protein-1.h-1 from DS1 to DS7, despite it slightly diminished at DS2. A significant decrease was finally registered (0.03 µg of hydrolyzed starch.mg protein-1.h-1) at DS8.
The βA activity (Figure 2c), as for αA activity, was in accordance with the pattern of starch fluctuations in inflorescences of the two cvs. (Figure 1a). In GW, the βA activity was constant between DS1 and DS3 (around 0.08 µg of formed maltose.mg protein-1.h-1) where the starch concentration did not fluctuate. A peak reaching 0.14 µg of formed maltose.mg protein-1.h-1 was observed at DS4, corresponding to the onset of starch hydrolysis. The activity was then declined between DS5 and DS7 whereas it increased at DS8 to reach 0.14 µg of formed maltose.mg protein-1.h-1, in parallel with starch degradation. In PN, a huge peak reaching 0.21 µg formed maltose.mg protein-1.h-1 was detected at DS1, corresponding to the simultaneous strongest mobilization of starch. Afterwards, the activity was not significantly modified until DS5, then slowly increased until fruit set (0.13 µg of formed maltose.mg protein-1.h-1), in accordance with starch degradation.
The SPS activity had the same pattern during the flower development in the both cvs. (Figure 3a) and was poorly correlated to sucrose variations (Figure 1b). The SPS activity was quite constant during the development, ranging approximately at 0.15 µg formed sucrose mg.protein-1.h-1. A temporary increase, by 3 and 6 fold in GW and PN respectively, was noticed at DS6.
The SSs activity had different patterns in the two cvs. (Figure 3b). While no activity was measured at DS1, DS5, DS7, and DS8 in GW, a huge peak (0.172 ± 0.050 µg formed sucrose mg.protein-1.h-1) was registered at DS2, corresponding to a simultaneous increase of sucrose concentrations (Figure 1b). In PN, the SSs activity was 0.167 ± 0.020 µg formed sucrose.mg protein-1.h-1 at the onset of flower development. Then, it declined during the following steps until DS3, which could be correlated with a decreased of sucrose contents (Figure 1b). At DS4, a peak of the SSs activity (0.140 ± 0.018 µg formed sucrose.mg protein-1.h-1), followed by a significant increase of sucrose content (Figure 1b). Thereafter, the SSs activity slightly diminished and was completely nil at DS8.
The sucrose cleavage was assayed by measuring activities of SSd (Figure 3c), WB Inv (Figure 3d), and Cy Inv (Figure 3e). The SSd activity fluctuated oppositely to sucrose content in both cultivars (Figure 3c). In GW, the SSd activity declined by 75% between DS1 (0.4 ± 0.09 µg degraded sucrose mg.protein-1.h-1) and DS3 (0.07 ± 0.02 µg degraded sucrose mg.protein-1.h-1), whereas the sucrose was accumulated in the meantime (Figure 1b). A peak of the SSd activity was registered at DS4, reaching 0.60 ± 0.02 µg degraded sucrose mg.protein-1.h-1, concomitantly with a sucrose degradation. A second peak (0.51 ± 0.08 µg degraded sucrose mg.protein-1.h-1) was finally observed at DS7. In PN inflorescences, the SSd activity presented two peaks at DS1 and DS4, corresponding respectively to 0.71 ± 0.16 and 0.42 ± 0.11 µg degraded sucrose.mg protein-1.h-1 and coinciding with a weak sucrose content (Figure 1b). The activity of SSd in PN was parallel to the SSd activity observed in GW from DS5 to DS8 (Figure 3c).
The cleavage of sucrose by invertases may occur either in the cell wall (WB Inv) or in the cytosol (Cy Inv). The WB Inv activity poorly fluctuated during the inflorescence development (Figure 3d). In GW, the activity was effective but constant, ranging approximately at 1 mg degraded sucrose.mg protein-1.h-1, from DS1 to DS5, then progressively increased up to 2.55 ± 0.52 µg degraded sucrose.mg protein-1.h-1 at DS8. Similar variation was observed in PN inflorescence. The WB Inv activity in PN did not coincide with the sucrose content at DS2 (Figure 1b).
The Cy Inv activity was lower than WB Inv and had globally similar patterns in the two cvs. (Figure 3e). The Cy Inv activity was not really correlated with the sucrose content variations except at DS3 (Figure 1b). At that time, the Cy Inv activity showed a temporary peak, reaching respectively 0.72 ± 0.17 and 0.35 ± 0.05 µg degraded sucrose.mg protein-1.h-1 in GW and PN. The Cy Inv activity progressively increased until from DS5 to the onset of fruit development, reaching the highest values at DS7 in PN (1.03 ± 0.22 µg degraded sucrose.mg protein-1.h-1) and DS8 in GW (1.05 ± 0.09 µg degraded sucrose.mg protein-1.h-1). In PN inflorescences, the Cy Inv decreased to 0.35 ± 0.10 µg degraded sucrose.mg protein-1.h-1 at DS8.
In grapevine inflorescences, both the development of reproductive organs and the carbohydrate metabolism are different in the flower-abscission sensitive GW and the non-sensitive PN. Indeed, the ontogenesis of reproductive organs is not synchronous in GW and PN cvs. Since both female and male meiosis occurred earlier in PN than in GW .
Starch and sucrose related enzyme activities were assayed in grapevine inflorescences during the development of flower growing in the vineyard for the first time. Our results showed that carbohydrate contents evolved during the development in the two cvs. In general, starch content decreased slowly and continually whereas the sucrose content increased through the first steps of the flower development before a decrease starting from the beginning of the flowering process.
In both cvs., the starch level variations were closely correlated with both enzyme activities. In GW inflorescences, the starch content was not really linked to the StSy activity but it was concomitant with the α-amylase activity and inversely linked to the β-amylase activity during the four first steps, then a tendency reversal occurred. The situation is different in PN since the variation of starch content was closely associated with enzyme activities, except with the β-amylase activity at DS2. Our results are in accordance with earlier results obtained in maize. Indeed, fluctuations of the starch content in maize ovaries are strongly related to the total amylase activity from 5 days before pollination to 2 days after . Moreover, it was already noticed that the starch content in PN could be correlated with the StSy activity in contrast to GW, leading the authors to suggest that although a similar starch concentration, the regulation of starch synthesis was different in inflorescences of the two cvs. Obtained from the artificial fruiting cutting model .
In both cvs., fluctuations of the sucrose in inflorescences during the flower development is consistent with activities of the three tested sucrose degradation enzymes, with a better correlation in PN. Indeed, fluctuations in the sucrose content were coherent with the SSd activity. In GW and PN inflorescences, each increase/decrease of the SSd activity coincided with a decrease/increase of the sucrose level. Moreover, the continual increase of Cy Inv and WB Inv activities during the last steps of the flower development also coincided with the low sucrose content in inflorescences of both cvs. In rice and wheat anthers, the SSd activity, except in wheat at the anthesis where the stimulation of SSd activity induces a strong decrease of sucrose levels . In grapevine, Sawicki et al. , already noticed a better correlation between activities of sucrose degradation enzymes and sucrose content in PN, compared to GW. These authors suggested that the higher degradation of sucrose in PN inflorescence around the female meiosis stage induced higher contents of hexose.
In the inflorescence of both cvs., activities of sucrose synthesizing enzymes do not have the same influence. Indeed, the SPS activity does not seem to interfere with sucrose variations, as well as in leaves of wheat . Nevertheless, the SSs activity might act in synergy with lower activities of sucrose degrading enzymes (SSd, invertases) during the first steps of development in GW inflorescences, explaining the sucrose increase observed at the beginning of “separated cluster” stage in this cultivar.
It appeared that in grapevine inflorescences, the sucrose was more degraded from the “flower separating” stage. Our results exhibit a significant enhance of both invertase (Cy and WB) activities at this stage. Moreover, at the “flower separating” stage, the chlorophyll concentration regularly diminishes leading to a decrease of net C02 assimilation and to the arrest of net positive photosynthesis at the fruit set for both GW and PN inflorescences [16,54,]. In the grapevine, during the flower development, inflorescences import carbohydrates and export photoassimilates . Consequently, sugar contents fluctuate differently according to the metabolism of the cultivar and inflorescences become a sink for carbohydrates from BBCH57 stage. It was already reported that the leaf photosynthetic rates are lower in GW than in PN  and that inflorescences have shown fluctuations in the photosynthetic activity during the flower development [6,26,27].
In grapevine, the accumulation of carbohydrates in berries begins during the maturation (Mullins et al. 1992). The sucrose is thus hydrolyzed, leading to an equal concentration in glucose and fructose [55,56]. It has been demonstrated that the activity of sucrose degrading enzymes in berry is stimulated at the fruit set and further increases until veraison [55,57]. In accordance, our results exhibit an increase in Cy Inv and WB Inv activities from the flowering till the fruit set.
During the flower development, variations of inflorescence enzyme activities between GW and PN can be connected with their differences in sugar contents. Indeed, the pool of available hexoses in developing inflorescences is higher in the PN than in the GW . Moreover, differences observed in the regulation of both cvs. May explain the lower sensitivity to flower abscission in PN under stress conditions [1,18] and the higher fruit set in GW under optimal conditions . Finally, the significant increase of sucrose degrading enzyme activities such as SSd, Cy Inv, and WB Inv during the last steps of the flower development may be interpreted as the first sign of the strong physiological modifications that occurs in the ovaries between the fertilization and the onset of fruit formation. This transition is reflected by both the positive photosynthesis in the inflorescence  and the early development of berries [58-60].
The authors would like to acknowledge the Conseil Interprofessionnel du Vin de Bordeaux, ONIVINS, Mumm-Perrier-Jouët Company and Reims métropole for their financial supports.
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