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2010. Plant Management Network. This article is in the public domain.
Accepted for publication 17 December 2009. Published 17 March 2010.

Differentiating Phytophthora ramorum and P. kernoviae from Other Species Isolated from Foliage of Rhododendrons

T. L. Widmer, USDA-ARS, Foreign Disease-Weed Science Research Unit, 1301 Ditto Avenue, Fort Detrick, MD 21702

Corresponding author: T. L. Widmer.

Widmer, T. L. 2010. Differentiating Phytophthora ramorum and P. kernoviae from other species isolated from foliage of rhododendrons. Online. Plant Health Progress doi:10.1094/PHP-2010-0317-01-RS.


Phytophthora species are among plant pathogens that are the most threatening to agriculture. After the discovery of P. ramorum, surveys have identified new species and new reports on rhododendrons. Based upon propagule production, morphology, and colony growth, a dichotomous key was produced that can differentiate P. ramorum and P. kernoviae from other species known to be pathogenic to aerial plant parts of rhododendrons. These distinctions were made without molecular tools and wide-ranging variables such as propagule sizes and can be made without the need for a large culture collection.


The discovery of Phytophthora ramorum as an invasive pathogen has prompted an increase in surveys for Phytophthora spp. resulting in the identification of several new species. Since 1999, P. foliorum (13), P. gonapodyides (26), P. hedraiandra (28,29), P. hibernalis (5), P. inflata (31), P. insolita (31), P. kernoviae (7), P. ramorum (37), and P. tropicalis (22) have all been newly described on Rhododendron spp. This is in addition to the previously known P. cactorum (11,29,35), P. cambivora (11,35), P. cinnamomi (11), P. citricola (11,29,35), P. citrophthora (29), P. heveae (11), P. nicotianae (synonym = P. parasitica) (11), and P. syringae (11). With quarantine regulations in effect for P. ramorum and concerns about the importation of P. kernoviae, which is known currently only in Great Britain and New Zealand, to North America, it is important to be able to identify clearly these two species and differentiate them from other Phytophthora spp. that attack leaves and stems of rhododendrons.

Before the advancement of molecular techniques, keys based upon morphological features were used to differentiate species. However, an often ambiguous overlapping of propagule size and the training needed to identify certain features made confident identification difficult. In addition, a good culture collection is needed for comparison purposes. With the advancement of molecular techniques, separation and identification of species is becoming more reliable. However, sequencing may not always result in clear distinctions when analyzing species that are closely related and other molecular tests may not be specific for an individual species (10). In addition, new Phytophthora species are being discovered frequently and there is no assurance that the current "ramorum-specific" primers will not react with these new species (30). This has already been observed with P. hibernalis (5) and P. foliorum (13). More importantly, not all laboratories have easy access to these molecular tools and it can be time consuming and expensive to send samples to more equipped laboratories. Osterbauer and Trippe (27) compared diagnostic protocols for P. ramorum on rhododendron leaves and found 16% of their samples were PCR negative, but culture positive. They also found 19% of their samples were PCR positive, but culture negative. This may be partially accounted for by the fact that PCR will also detect spores that are nonviable or are in some state of dormancy. In a related study, Sutton et al. (30) concluded that culturing was the single most reliable method for detection of P. ramorum. Thus, a method for confident identification based upon stable and simple morphological characteristics needs to be updated.

Several synoptic keys have been published to identify Phytophthora spp. (14,20). Recently, Gallegly and Hong (15) compiled 60 known Phytophthora spp. together with photographs and DNA fingerprinting. Despite this information, identification through morphology is considered difficult because features are variable and often overlap within species (14). In addition, some recently described species, including P. ramorum and P. kernoviae, were not included in these older keys. Currently, United States Federal regulations require that all program samples (i.e., collected during surveys of nurseries in the regulated states of California, Washington, and Oregon, or in nurseries of another state as a result of a trace forward) that are symptomatic be sampled and tested for P. ramorum (34). Samples will then be considered positive for P. ramorum based upon results of a positive PCR or positive culture. Survey and diagnostic samples from nurseries in non-regulated states or not part of a trace forward or trace back can be identified based on morphology and or DNA sequence. It is the attempt of this study to present morphological characteristics that can be used to differentiate P. ramorum and P. kernoviae from other Phytophthora spp. pathogenic to rhododendron leaves and stems. This key will be especially useful to diagnostic and extension laboratories that receive rhododendron leaf samples and are not required to confirm identification through PCR. It could also be useful for differentiating these species from any woody plant.

Species Characteristics

Isolates used. Phytophthora species known to be pathogenic to Rhododendron were identified through a literature search. Cultures of these Phytophthora spp., listed in Table 1, were obtained from various researchers and maintained on 20% clarified V8 agar. Observations were based on examinations of two isolates from each species having, if possible, at least one of the isolates collected from rhododendron. It was justified to use only two isolates since the primary diagnostic features used in this study (e.g., sexual type, sporangia characteristics, etc.) are stable characteristics that are used to define the species and it was sufficient in a recent publication on Phytophthora spp. identification (15). Isolates of P. inflata and P. insolita could not be obtained and characteristics were based solely upon the literature (2,14,17). An unidentified Phytophthora taxon labeled Pgchlamydo, isolated from Rhododendron (28), was not included in this study since it has not been officially described. Other species isolated only from rhododendron roots (P. lateralis, P. cryptogea, and P. megasperma) (14,21) were not included in this study.

Table 1. List of Phytophthora spp. isolates used in this study, their origin, original host material, and source.

Phytophthora spp. Isolate Origin Host Sourcex
P. cactorum Benson JCW1 NC Rhododendron MB (35)
P. cactorum Hamm 348 WA Douglas Fir PH (N/A)
P. cambivora Benson AJH5 NC Rhododendron MB (35)
P. cambivora Benson HCW3 NC Unknown MB (N/A)
P. cinnamomi Benson 2357 NC Azalea MB (N/A)
P. cinnamomi 3267 CA Walnut GB (33)
P. citricola Benson AJH6 NC Rhododendron MB (35)
P. citricola Benson FKP4 NC Rhododendron MB (N/A)
P. citrophthora Reeser 01-02 OR Rhododendron JP (35)
P. citrophthora 3E5 VA Irrigation water CH, MG (15,23)
P. foliorum LT192 TN Rhododendron KL (13)
P. foliorum LT1223 CA Rhododendron KL (13)
P. gonapodyides Pgon26 SC Soil JH (N/A)
P. gonapodyides Pgon56 FL Soil JH (N/A)
P. hedraiandra MN832003 MN Rhododendron RB (28)
P. hedraiandra MN1522003 MN Rhododendron RB (GenBank DQ139806)
P. heveae Reeser PC97-251 OR Rhododendron JP (33)
P. heveae HW228 NC Rhododendron SJ (N/A)
P. hibernalis ATCC 32995 CA Citrus sinensis MC (25)
P. hibernalis ATCC 64708 New Zealand Aquilega vulgaris ATCC (25)
P. kernoviae CSL 2378 England Rhododendron KH (GenBank DQ002011)
P. kernoviae ICMP 14761 New Zealand Annona cherimola TR (GenBank EU909457)
P. nicotianae Pn21DJM FL Periwinkle FM (N/A)
P. nicotianae 362 DE Solanum tuberosum RM (32)
P. ramorum Pr-52 CA Rhododendron DR (13,25)
P. ramorum PRN-1 the Netherlands Rhododendron SW (23)
P. syringae Kalmia-1 OR Kalmia latifolia JP (13,25)
P. syringae Kalmia-2 OR Kalmia latifolia JP (13,25)
P. tropicalis 31C9 VA Rhododendron CH (22)
P. tropicalis SR10 VA Soil SJ (N/A)

 x Name of originator followed by a reference to the molecular identification in parenthesis (N/A = not available and was identified only on morphology or through RLFP patterns). ATCC = American Type Culture Collection; CH = Chuan Hong; DR = Dave Rizzo; FM = Frank Martin; GB = Greg Browne; JH = Jaesoon Hwang; JP = Jennifer Parke; KH = Kelvin Hughes; KL = Kurt Lamour; MB = Mike Benson; MC = Mike Coffey; MG = Mannon Gallegly; RB = Robert Blanchette; RM = Robert Mulrooney; PH = Phil Hamm; SJ = Steve Jeffers; SW = Sabine Werres; TR = Tod Ramsfield.

Propagule inducement. Cultures of Phytophthora spp. were prepared in sterile 10% clarified V8 broth and placed in an incubator at 20°C, either under continuous light (3180 lux) or in the dark. The cultures were observed for the formation of propagules after 3 and 4 days. After 4 days, the cultures were rinsed three times with either sterile 0.1 mM MES buffer, pH 6.2 or sterile 1% soil extract. The cultures were placed back in the incubators either under light or dark at 20°C as they were before rinsing. One day after rinsing, the cultures were again observed for the formation of propagules (Table 2). Some species required longer for production of certain propagules. Caducity of sporangia was determined by a modified procedure described by Al-Hedaithy and Tsao (1). Four days after the sporangia had formed, the plates were sealed with Parafilm (Pechiney Packaging Co., Chicago, IL) and shaken vigorously for 10 sec. The species was determined to have obvious caducity if detached sporangia with consistent pedicel lengths were observed in the solution. The species was rated as noncaducous or not to have obvious caducity if very few sporangia (< 10%) were released and the pedicel lengths were not consistent (1). Photographs were taken of each propagule type that was observed in this study (Figs. 1 to 15).


Fig. 1. Phytophthora cactorum (A) oospore; (B) sporangium. Bar = 10 µm.


Fig. 2. Phytophthora cambivora (A) hyphal swellings. Bar = 100 µm; (B) sporangium. Bar = 10 µm.


Fig. 3. Phytophthora cinnamomi (A) chlamydospore. Bar = 10 µm; (B) sporangium. Bar = 10 µm; (C) hyphal swellings. Bar = 100 µm.


Fig. 4. Phytophthora citricola (A) oospore; (B) sporangium. Bar = 10 µm.


Fig. 5. Phytophthora citrophthora sporangium. Bar = 10 µm.



Fig. 6. Phytophthora foliorum (A) oospore; (B) sporangium. Bar = 10 µm.


Fig. 7. Phytophthora gonapodyides (A) chlamydospores; (B) sporangium. Bar = 10 µm.


Fig. 8. Phytophthora hedraiandra (A) oospore; (B) sporangium. Bar = 10 µm; (C) mycelium after 7 days growth on V8 agar at 4°C. Bar = 100 µm.


Fig. 9. Phytophthora heveae (A) oospore; (B) sporangium; (C) hyphal swelling. Bar = 10 µm.


Fig. 10. Phytophthora hibernalis (A) oospore; (B) sporangium. Bar = 10 µm.


Fig. 11. Phytophthora kernoviae (A) oospore; (B) sporangium. Bar = 10 µm.


Fig. 12. Phytophthora nicotianae (A) chlamydospore; (B) sporangium. Bar = 10 µm.


Fig. 13. Phytophthora ramorum (A) chlamydospores; (B) sporangium. Bar = 10 µm.


Fig. 14. Phytophthora syringae (A) oospore; (B) sporangium. Bar = 10 µm.


Fig. 15. Phytophthora tropicalis (A) chlamydospore; (B) sporangium. Bar = 10 µm.

Table 2. Propagule type of different Phytophthora spp. observed in liquid cultures grown at 20°C.

Species Condition Growth in V8 brothw Washing solutionx
3 days 4 days 1 day MES 1 day SE
P. cactorum Light Spy Sp+ Sp+, Oog Sp+, Oog
Dark Oog+ Oog+ Sp, Oog+ Sp, Oog+
P. cambivora Light M M Sp Sp+
Dark HS HS HS HS, Sp
P. cinnamomi Light Ch+, HS+ Ch+, HS+ Ch+, HS+ Ch+, HS+, Sp
Dark Ch+, HS+ Ch+, HS+ Ch+, HS+ Ch+, HS+, Sp
P. citricola Light M M Sp+ Sp+
Dark M Oog Oog Sp, Oog
P. citrophthora Light Sp+ Sp+ Sp+ Sp+
Dark M Sp Sp Sp+
P. foliorum Light M Oog Oog+ Sp, Oog+
Dark M Oog+ Oog+ Sp, Oog+
P. gonapodyides Light M M Ch+, Sp Sp
Dark M M Ch+, Sp Sp
P. hedraiandra Light Sp+ Sp+ Sp+ Sp+
Dark Oog+ Oog+ Oog+, Sp Oog+, Sp
P. heveae Light Oog Oog+, Sp Oog+ Oog+, Sp
Dark Oog+ Oog+ Oog+ Oog+
P. hibernalis Light M M Sp Sp+
Dark M M Oog Sp, Oog
P. kernoviae Light Sp Sp+ Sp+ Sp+
Dark M Oog+ Sp, Oog+ Sp+, Oog+
P. nicotianae Light Sp Sp+ Ch+, Sp+ Ch+, Sp+
Dark M Ch, Sp Ch, Sp Ch, Sp
P. ramorum Light M Chz, Sp+ Sp+ Sp+
Dark M Chz, Sp Sp+ Sp+
P. syringae Light M M Sp+, Oog+ Sp+, Oog+
Dark M Oog+ Sp, Oog+ Sp+, Oog+
P. tropicalis Light Sp+ Sp+ Sp+ Sp+
Dark M M Sp Ch, Sp+

 w Propagule type observed after growing for 3 or 4 days in 10% V8 broth at 20°C under continuous light or in the dark.

 x Propagule type observed after growing in 10% V8 broth for 4 days, washing three times in either 0.1 mM MES buffer, pH 6.2 or 1% sterile soil extract (SE), and incubating for 1 day at 20°C under continuous light or in the dark.

 y Propagule type: Ch = chlamydospores; HS = hyphal swellings; M = mycelium only; Oog = oogonia; Sp = sporangia. (+) denotes abundant production of corresponding propagule.

 z Chlamydospores of P. ramorum were first observed 6 days after inoculation in 10% V8 broth.

Colony growth at different temperatures. To confirm previous reports of growth of the Phytophthora spp. at different temperatures, V8 agar plates with a plug from an actively growing colony were placed on a thermogradient plate (an aluminum plate with a hot water bath at one end and a cooling bath at the other end) at 2°C intervals from 4° to 10°, 20°, and 26° to 32°C in darkness (25). The desired temperature of the agar medium was confirmed daily by touching the Type-K probe of an Omega Model HH21 Microprocessor Thermometer (Omega Engineering, Inc.) onto the surface of a V8 agar plate. Cultures were considered to have positive growth if mycelium was observed on the V8 agar plate after 7 days. This was repeated once for each isolate. Although a majority of isolates tested in this study grew within the temperature range reported in the literature (3,7,12,13,14,37), there were some exceptions. Isolates of P. cambivora, P. cinnamomi, P. citricola, and P. citrophthora all grew within a narrower temperature range than previously reported (14). The isolate of P. heveae used in this study grew at a much lower minimum temperature (4°C) and a lower maximum temperature (26°C) than previously reported (14). Based on these results, growth at different temperatures can be isolate dependent and so was not used as a primary characteristic in this study, except in the case with P. syringae separating it from P. citricola, P. foliorum, and P. inflata. Phytophthora syringae is reported to have a maximum temperature of growth of 23 to 25°C (14), which was confirmed in this study, while the other three species grow well above 28°C.

Colony morphology on agar media. Colony morphology of the species was compared by growing the isolates on carrot agar, Rye A agar, and 20% clarified V8 agar at 20°C in the dark (14). Photographs of the plates were taken when the colonies reached the edge of the plates (Fig. 16). There is some discussion as to the usefulness of colony patterns for the identification of Phytophthora spp. Waterhouse (36) remarks that patterns should be considered as a taxonomic aid, but Erwin and Ribeiro (14) demonstrate that variability of colony types among isolates of different species make this characteristic not useful for identification beyond supplementary purposes. A majority of papers describing new species [e.g. (7,37)] include colony patterns in the description and so were included in this study for possible reference. Some species had very distinct patterns on all three media types. For example, P. citricola showed rosaceous patterns (Fig. 16D) while P. syringae was very distinctly stellate (Fig. 16N) and P. hedraiandra was petallate (Fig. 16H). Phytophthora heveae ranged from stellate on V8 and Rye A agar to rosaceous on carrot agar (Fig. 16J).


Fig. 16. Colonies of: (A) Phytophthora cactorum; (B) P. cambivora; (C) P. cinnamomi; (D) P. citricola; (E) P. citrophthora; (F) P. foliorum; (G) P. gonapodyides; (H) P. hedraiandra; (I) P. heveae; (J) P. hibernalis; (K) P. kernoviae; (L) P. nicotianae; (M) P. ramorum; (N) P. syringae; and (O) P. tropicalis grown on 20%V8 agar (top row), Rye A agar (middle row), and carrot agar (bottom row).


Discrepancies from previous reports. Although the majority of results in this study agreed with previous reports, several important differences were noted. In the original description (13), P. foliorum sporangia were reported as caducous. However, in this study, P. foliorum sporangia were not rated as caducuous. Although slightly more than 10% of the sporangia detached into the solution after shaking, the pedicel lengths were highly variable ranging from no pedicel to long detached hyphae (data not shown). This is an important criteria for caducity based upon a study by Al-Hedaithy and Tsao (1). There is also some discrepancy in the literature concerning the caducity of P. heveae. Erwin and Ribeiro (14) described caducous sporangia with a pedicel length less than 10 µm, whereas Gallegly and Hong (15) observed noncaducous sporangia. In this study, very few sporangia detached after shaking and obvious caducity was not observed, based upon the criteria mentioned above.

Another notable difference was the production of chlamydospores in the P. gonapodyides cultures (Fig. 7A). Previous studies have reported other P. gonapodyides isolates to produce chlamydospores (18), but Erwin and Ribeiro (14) describe this species as producing no chlamydospores or hyphal swellings. If P. gonapodyides is suspected, but no chlamydospores are formed, then according to the key (Fig. 17) it would fall under the same grouping as P. citrophthora. Phytophthora gonapodyides can be differentiated from P. citrophthora based upon the papillation type of the sporangia, where P. gonapodyides is non-papillate and P. citrophthora is papillate. Production of chlamydospores has also been used as a distinguishing characteristic between P. gonapodyides and the unidentified Phytophthora taxon labeled Pgchlamydo (8). However, at this time it is unclear as to whether production or lack of chlamydospores or hyphal swellings is enough to separate these two species. Greslebin et al. (16) analyzed isolates that matched 100% with P. gonapodyides sequences, but produced hyphal swellings in culture. At the time of this study, the isolates used were identified as P. gonapodyides. But, as the classification of Phytophthora spp. evolves, based on new molecular techniques, this identification may change.


Fig. 17. Dichotomous key using stable characteristics to differentiate Phytophthora spp. that are known to be pathogenic to foliar plant parts of Rhododendron spp.

Differentiating P. ramorum and P. kernoviae. Based upon the characteristics outlined below, it is possible to differentiate P. ramorum and P. kernoviae from other known species that attack the stems and leaves of rhododendrons. A dichotomous key was designed to separate these two species based upon morphological characteristics (Fig. 17).

Oospore production is the first characteristic used to separate P. ramorum and P. kernoviae from each other. Phytophthora kernoviae is homothallic and a single culture produces abundant oospores. On the other hand, P. ramorum is heterothallic and is difficult to produce oospores even when the two mating types are combined in a laboratory (6). Oospores of P. ramorum have never been observed in nature (19).

If oospores are not formed in single isolate cultures, the lack of chlamydospore production will distinguish P. citrophthora and P. cambivora from other heterothallic species. Some P. citrophthora isolates from cacao in Brazil were reported to produce chlamydospores (14). No chlamydospores were observed in the P. citrophthora isolates used in this study. A good characteristic of P. ramorum is their very large and distinct chlamydospores. However, there is a range of chlamydospore sizes that could overlap other species and so someone who is unfamiliar with P. ramorum and does not have cultures of other species to compare it to, may not be able to confirm the identity. Thus, other characteristics must be used to further distinguish P. ramorum from other species. Phytophthora cinnamomi can be separated from the group that produces chlamydospores based upon its distinct hyphal swellings (Fig. 3B) and that it does not produce abundant sporangia, if any, in liquid culture (9). Papillae type of the sporangia is then used to differentiate the other species. Phytophthora ramorum has semi-papillate sporangia while the other species in this group are either papillate or non-papillate. Sometimes, it is difficult to distinguish papillate from semi-papillate sporangia, so other characteristics may be useful to separate P. ramorum from P. nicotianae and P. tropicalis. All three species produce chlamydospores, but as mentioned above, P. ramorum chlamydospores are very large on average compared to the other two species. The average chlamydospore diameter for most isolates of P. ramorum is 46 to 60 µm (37), which compare to P. nicotianae and P. tropicalis chlamydospores that are 30 µm and 27 to 34 µm, respectively (15). Phytophthora nicotianae can be differentiated from P. ramorum and P. tropicalis because it produces non-caducous sporangia. If papillate type and chlamydospore size is in question, P. tropicalis can be differentiated from P. ramorum based on its colony growth at higher (> 30°C) temperatures, compared to maximum temperature growth at 26 to 30°C for P. ramorum (37).

Phytophthora kernoviae can be separated from other homothallic Phytophthora spp. based upon three characteristics. Firstly, P. kernoviae has papillate sporangia that are shared with P. heveae, P. cactorum, and P. hedraiandra. Secondly, P. kernoviae and P. heveae have amphigynous antheridia compared to paragynous antheridia characteristic of P. cactorum and P. hedraiandra. However, in the original description of P. hedraiandra (12), antheridia were reported to be occasionally amphigynous. Descriptions in the literature (14) where the position of the antheridium can be occasionally amphigynous or paragynous is the reason that this characteristic is not used to separate other homothallic species. A backup characteristic to separate P. kernoviae from P. cactorum or P. hedraiandra is the pedicel length of the caducous sporangia. Phytophthora kernoviae has a medium length pedicel with a range of 5 to 19 µm (7) compared to P. hedraiandra and P. cactorum, which have a short pedicel length less than 2 and 4 µm, respectively (12,14). This is clearly shown in Figures 1B, 8B, and 11B. In addition, P. kernoviae has very little colony growth at 26°C, while P. cactorum grows well at 28°C and P. hedraiandra can even grow at 30°C. Finally, the lack of hyphal swellings in P. kernoviae cultures differentiates it from P. heveae, where they are evident (Fig. 9C). Other characteristics also may be helpful in differentiating these two species. Although conflicted in the literature, as mentioned above, P. kernoviae has obvious caducous sporangia compared to P. heveae, which are ambiguous. Another distinguishing characteristic is that P. heveae oospores are markedly aplerotic (14,15), whereas oospores of P. kernoviae are plerotic (7). This characteristic, however, may be difficult to discern.

Differentiating Other Species with Closely Related Characteristics

In the presented dichotomous key, there were two sets of species that could not be differentiated based upon one characteristic. To distinguish these species from one another, the combination of several features were used. These characteristics included growth at different temperature extremes, colony patterns, oospore morphology, and propagule production that were included in the synoptic key by Ho (20), but were noted to be variable within species.

Phytophthora citricola, P. foliorum, and P. inflata all have similar characteristics outlined in this study and are difficult to separate based upon a single one. To separate P. inflata, published results report the formation of intercalary hyphal swellings in aqueous cultures (14). Hyphal swellings have not been observed in P. citricola or P. foliorum cultures. In addition, colony morphology may provide further confidence in separating P. inflata from P. citricola and P. foliorum. Hall et al. (17) reported a pronounced stellate pattern of P. inflata on V8 agar in comparison to the petalloid colonies of P. citricola and P. foliorum observed in this study (Figs. 16D and 16F). The abundance of sporangia produced in liquid culture may be the best distinguishing characteristic between P. citricola and P. foliorum. Abundant P. citricola sporangia formed in cultures rinsed with soil extract or MES buffer and kept under continuous light, whereas P. foliorum produced very few sporangia, regardless of the treatment or condition (Table 2). Donahoo et al. (13) also reported difficulties producing large amounts of P. foliorum sporangia. Colony growth at lower temperatures is not a reliable characteristic to separate P. foliorum and P. citricola. In this study, P. foliorum grew slightly at 4° and 6°C, whereas the minimum growth temperature for P. citricola was 8°C. However, Erwin and Ribeiro (14) reported the minimum growth temperature for P. citricola is 3°C, which demonstrates that this characteristic may be dependent upon which P. citricola group the isolate fall under. Gallegly and Hong (15) separated P. citricola into three distinct groups based upon single-strand conformation polymorphism (SSCP) analysis but could not define physical characteristics to distinguish them.

Likewise, it is very difficult to separate P. hedraiandra from P. cactorum (12,24). Some of the unique physical characteristics of P. hedraiandra mentioned in the literature (12), such as predominantly sessile antheridia, the absence of tangled hyphae below the antheridia, and the larger oospores are not easy to identify. In this study, P. hedraiandra could be distinguished from P. cactorum based upon colony morphology growing on agar plates. At 20°C, P. hedraiandra produced a definite petalloid colony compared to the more cottony colony of P. cactorum (Figs. 16H and 16A). This was more pronounced on the Rye A agar plates. In addition, culturing in an incubator under artificial light inhibited the formation of oogonia in liquid cultures of P. hedraiandra 1 day after rinsing with MES buffer or soil extract, while oogonia formed in P. cactorum under the same conditions (Table 2).

Finally, P. insolita differs from other homothallic species in this study by producing nonpapillate, noncaducous sporangia (14), and sexual structures void of antheridia (15). In addition, this species produces chlamydospores (2), which is a unique characteristic among the other homothallic species in this study.

In conclusion, the data presented here can be useful for differentiating P. ramorum and P. kernoviae from other Phytophthora spp. that are pathogenic to aerial plant parts of rhododendrons. If P. ramorum or P. kernoviae are suspected, based upon the data presented here, it is important to verify the identification through approved and accepted molecular techniques. However, the key provided in this study will be useful in assisting diagnostic labs and extension agents that may not have the tools or resources available to use molecular techniques in identifying Phytophthora spp. for screening purposes.

Acknowledgments and Disclaimers

The author would like to thank Mike Benson, Robert Blanchette, Mike Coffey, Mannon Gallegly, Chuan Hong, Kelvin Hughes, Jaesoon Hwang, Steve Jeffers, Kurt Lamour, Frank Martin, Robert Mulrooney, Jennifer Parke, Dave Rizzo, and Paul Tooley for providing the isolates, Marie Carras for reviving the isolates from frozen cultures, and Stephen Dodge for verification of the key by identifying unknown isolates. Special thanks to Mannon Gallegly for his review of the manuscript and helpful suggestions and the anonymous reviewers for their critical reviews to make this a better manuscript. All laboratory studies were conducted in a quarantine facility under permit from APHIS.

Mention of a trademark, proprietary product, or vendor does not constitute a guarantee or warranty of the product by the USDA and does not imply its approval to the exclusion of other products or vendors that also may be suitable.

Literature Cited

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