**Diseases Caused by Bacteria**

Bacteria are not major pathogens of chickpeas and lentils and there are
very few bacterial diseases reported for chickpeas and lentils. Of the
bacterial diseases reported, only limited information is available
describing the symptoms produced, the causal agent, disease cycle or
management practices. They are considered to be of minor importance and
are usually not a concern unless the plants are grown in high rainfall
areas or under irrigation. The following is a summary of the current
knowledge of bacterial diseases of chickpeas and lentils.

**Bacterial Blight and Damping-off**

Pre- and post-emergence damping-off as well as wilting of older
chickpeas plants is caused by the bacterial blight pathogen *Xanthomonas
campestris* pv. *cassiae*. This disease is characterized by water-soaked
lesions on the radicle and young root tissue which turns dark brown.
Water-soaked lesions can also appear on the leaf surface that progress
into dark brown lesions with chlorotic halos. Petiole infections will
result in brown lesions and defoliation. Over time infected tissues
appear to loose their structural integrity and disintegrate taking on a
soft rot appearance. While not a common problem for chickpea production,
this disease can have a significant impact on early planted chickpea
exposed to high temperatures and sporadic rain. *X. campestris* pv.
*cassiae* is a Gram-negative, rod-shaped, aerobic bacterium
approximately 0.8 x 1.4 μm in size with a single polar flagellum. It
produces characteristic yellow, mucoid and irregular shaped colonies on
nutrient rich media.

![](media/image1.jpeg){width="3.0in" height="2.3333333333333335in"}

Fig. 1. Bacterial blight of chickpea showing drying and defoliation of
leaves. (Courtesy ICRISAT)

**Bacterial Stem Canker**

Stem cankers, leaf spots and dieback are observed on chickpeas infected
with *Pseudomonas andropogonis*. The infected plants will produce few
blossoms resulting in reduced pod set. Complete plant defoliation can be
seen in severely infected plants. While infection of chickpea by *P.
andropogonis* is not common, there have been isolated outbreaks in
Australia and one report in the US. *P. andropogonis* is a strict aerobe
producing circular, white, smooth colonies on rich media which do not
fluoresce on iron-deficient media. It is a Gram-negative rod
approximately 0.6 x 1.6 μm in size with a single polar flagellum.

**Pink Seed**

*Erwinia* *rhapontici* is a pathogen of both chickpeas and lentils
causing pink seed*.* The incidence of this pathogen is low and there
have been no studies to determine the impact of this pathogen on
lentils. However, there is evidence that infection of pea by *E.*
*rhapontici* reduces the seed size, seedling emergence and overall vigor
of the plant. While the physiological impact of this pathogen on its
host is minor, detection of pink seed can result in an economic loss to
the producer. Seed infected with *E.* *rhapontici* is pink in appearance
and the coloration is often mistaken for a pink-colored fungicide
treatment, reducing the quality of the seed lot. If a high percentage of
pink pea seed is detected, the lot will mistakenly be graded as having
pesticide contamination and can not be used for human consumption. *E.*
*rhapontici* is a facultative anaerobe producing pale pink colonies on
nutrient rich media.

**Bacterial Root rot**

Root rot of lentils is caused by *Pseudomonas radiciperda*. This disease
is characterized by the presence of dark oblong, lesions at the base of
the stem and discoloration of the vascular system beneath the lesions.
Monocropping of lentil is reported to exacerbate the disease with
potential for complete destruction of a crop within three years. Studies
indicate that most lentil varieties are susceptible to the bacterium.
There are some lentil germplasm collections that contain accessions that
are more resistant to the bacterium than others. *P. radiciperda* is a
Gram-negative, aerobic rod-shaped bacterium that produces smooth white
colonies on rich media and is unable to fluoresce on iron depleted
media.

Host range studies have determined that the bacterial pathogens
*Rhodococcus faciens* and *Xanthomonas campestris* pv. *phaseoli* are
able to cause disease on chickpea and lentils, respectively. *X.
campestris* pv. *phaseoli* can produce leaf spot symptoms on lentils as
result of artificial inoculations, however, this pathogen has not been
reported to cause disease under agronomic conditions. *X. campestris*
pv. *phaseoli* is a rod-shaped aerobic bacterium producing
characteristic yellow, mucoid colonies on rich nutrient media.
*Rhodococcus (Corynebacterium) faciens* is capable of causing fasciation
and stunting on wide range of host plants. Inoculation of chickpea
seedlings with *R. faciens* result in increased shoot and root
proliferation. *R. faciens* produces chrome-yellow to cream colored
colonies on nutrient agar. *R. faciens* is a rod-shaped, Gram-positive,
non-motile bacterium that requires thiamine for growth.

Management

General management practices for bacterial diseases include rotation of
planting fields and planting seeds free of contamination by pathogenic
bacteria. Bacterial diseases are generally favored by warm and humid
conditions. In areas where bacterial diseases are frequent and severe,
cultural practices that reduce relative humidity in the microenvironment
under canopy such wide-row spacing and/or escape warm weather such as
early planting can help reduce incidence of bacterial diseases.

Caruso, F. L. 1984. Bacterial blight of chickpea incited by *Pseudomonas
andropogonis*. Plant Dis. 68: 910-913.

Holt, J. G., Krieg, N. R., Sneath, P. H. A., Staley, J. T., and
Williams, S, T. 1994. Bergey\'s Manual of Determinative Bacteriology,
Williams & Wilkins. Baltimore. US. 9th ed. 787 p.

Huang, H. C., Erickson, R. S., Yanke, L. J., Hsieh, T. F., and Morrall,
R. A. A. 2003. First report of pink seed of lentil and chickpea caused
by *Erwinia rhapontici* in Canada. Plant Dis. 87: 1398.

Huang, H. C., and Erickson, R. S. 2002. Impacts of pink pea disease on
seed size, seedling emergence, and growth vigor. Can. J. Plant Pathol.
24:388.

Jacobs, S. E., and Mohanty, U. 1951. Studies in bacteriosis. XXVII.
Factors influencing infection by *Corynebacterium faciens*. Ann. Appl.
Biol. 38:237-245.

Javoronkova, I. P. (Mme). 1932. Bacterial root rot of red clover,
lucerne and lentils caused by *Bacterium radiciperda* n. sp. Bull. Plant
Protection, Leningrad 5:161-172.

Kore, S. S., and Nikitina, K. V. 1966. Investigations on bacterial leaf
spot disease of urd bean (*Phaseolus mungo*). Indian Jour. Mycology and
Plant Pathology 10:142-145.

Luzina, Z. A., and Nikitina, K. V. 1966. Bacterial infection of lentil.
Sel. Khoz. Biol. 1:277-297.

Mohanty, U. 1951. *Corynebacterium fasciens* (Tilford) Dowson; its
morphology, physiology, nutrition and taxonomic position. Trans. Brit.
Mycol. Soc. 34:23-34.

Navaratnam, S. J., and Hayward, A. C. 1979. Bacterial blight of
chickpea. Aust. Plant Pathol. 8:18.

Putnam, M. L., and Miller, M. L. 2007. *Rhodococcus fascians* in
herbaceous perennials. Plant Dis. 91:1064-1076.

Rangaswami, G., and Prasad, N. N. A bacterial disease of *Cicer
arietinum* L. Indian Phytopathology 12:172-175.

(Prepared by B. K. Schroeder)

**Disease caused by a Phytoplasma**

**Phyllody of chickpea**

Phyllody is a minor problem in chickpea because of its infrequent
occurrence. The disease is caused by a leafhopper-transmitted
phytoplasma (formerly known as a mycoplasma-like organism or MLO) and
occurs both in Desi and Kabuli type chickpea cultivars. Chickpea
phyllody disease was first reported in 1959 from Coimbatore in Tamil
Nadu, India. It has been reported since then in Ethiopia, India and
Myanmar and most recently in Australia, Oman and Pakistan.

# Symptoms

Phyllody means transformation of floral parts into green leaf-like
structures (Figs. 1 and 2) and this is the most characteristic symptom
of the disease. The normally white to mauve calyx of flowers is small
and green or absent, whereas the sepals are enlarged. Ovaries generate
individual leaves or shoots with additional sterile, phylloid flowers
and elongated pedicels. However, the expansion of these structures and
ordinary leaves is less than normal, so that the overall width of
foliage on each branch is less than normal (Fig. 3). If infection occurs
early, pods are not produced after the onset of infection. If infection
is late, phyllody can be less pronounced and restricted to tops of
shoots and small sickle-shaped pods (Fig 2) with shriveled seed (Fig. 4)
may form. Infected plants have a scattered field distribution as for
viruses in chickpea. They are commonly stunted and bushy in appearance
and remain green after surrounding plants have matured (Fig 5). However,
depending possibly on phytoplasma strain and/or chickpea cultivar,
plants can also be vigorous though sterile and devoid of seed. Yield
losses are greater for vigorous plants because there is no compensatory
growth of fertile branches from neighboring plants.

# Causal agent

Chickpea phyllody is caused by at least two distinct leafhopper
transmitted phytoplasmas (uncultureable bacteria of class *Mollicutes*)
having high similarity to the 16SrII-B group in Oman and 16SrII-D in
Pakistan. The phytoplasma is a highly pleomorphic prokaryote devoid of
cell walls and ranges in size from 200-600 nm and consists of opaque,
low electron density cytoplasm that contain ribosome-like granules,
DNA-strand like structures and lack a nuclear membrane. The agent is
restricted to the phloem sieve tube cells in chickpea.

# Host range and epidemiology

Chickpea phyllody persists primarily in chickpea and the leafhopper
vectors. The principle vector of chickpea phyllody in India and Pakistan
is *Orosius albicinctus* (Fig. 6). Natural infection of other alternate
hosts with phytoplasma causing chickpea phyllody has yet to be
identified. However in India the causal agent of sesame phyllody disease
was reported to be transmissible to chickpea using the leafhopper *O.
albicinctus*. The disease agent can also be transmitted by grafting but
is not mechanically transmissible nor is it transmitted through seed.

# Management

The most effective management practice is to destroy weed reservoirs
located near the crop to reduce primary inoculum and discourage buildup
of leafhopper populations. The disease could be managed by spraying
systemic insecticides to eliminate leafhopper colonization within the
crop to reduce secondary spread. The disease symptoms can also be
suppressed temporally by foliar application of oxytetracycline
hydrochloride solution (500 ppm) at weekly intervals.

# Selected references

Akhtar, K. P., Shah, T. M., Atta, B. M., Dickinson, M., Jamil, F. F.,
Haq, M. A., Hameed, S., and Iqbal, M. J. 2008. Natural occurrence of
phytoplasma associated with chickpea phyllody disease in Pakistan - a
new record. Plant Pathol. (Doi: 10.1111/j.1365-3059.2007.01800.x)

Al-Saady, N. A., Al-Subhi, A. M., Al-Nabhani, A., and Khan, A. J. 2006.
First record of a Group 16SrII phytoplasma infecting chickpea in Oman.
Plant Dis. 90: 273.

Ghanekar, A. M., Manohar, S. K., Reddy, S. V., and Nene, Y. L. 1988.
Association of a mycoplasma-like organism with chickpea phyllody. Ind.
Phytopathol. 41: 462-464.

Saqib, M., Bayliss, K. L., Dell, B., Hardy, G. E. St. J., and Jones, M.
G. K. 2005. First record of a phytoplasma-associated disease of chickpea
(*Cicer arietinum*) in Australia. Australas. Plant Pathol. 34: 425-426.

(Prepared by K. P. Akhtar, F. F. Jamil and M. A. Haq)

**Figures**

![](media/image2.jpeg){width="2.3194444444444446in"
height="2.6395833333333334in"}

**Fig. 1.** Healthy and normal flowers (left) and abnormal green
structure (phyllody) on right. (Courtesy K. P. Akhtar)

![](media/image3.jpeg){width="2.8319444444444444in"
height="2.123611111111111in"}

**Fig. 2.** Healthy pod (left) and sickle shaped pods (right). (Courtesy
K. P. Akhtar)

![](media/image4.jpeg){width="2.176388888888889in"
height="2.421527777777778in"}

Fig. 3. Phyllody symptoms in desi chickpea as well as green deformed
flowers, the plant has leaves that are shortened and less spreading than
normal and leaflets that show marginal reddening. (Courtesy K. P.
Akhtar)

![](media/image5.jpeg){width="2.5881944444444445in"
height="1.9333333333333333in"}

**Fig. 4.** Healthy seeds (left) and abnormal degenerated seeds (right).
(Courtesy K. P. Akhtar)

![](media/image6.jpeg){width="3.167361111111111in"
height="2.3756944444444446in"}

**Fig. 5.** Conspicuously green diseased plant of phyllody symptom.
(Courtesy K. P. Akhtar)

# 

![](media/image7.png){width="3.5in" height="2.6347222222222224in"}

Fig. 6. Leafhopper *Orosius albicinctus­*, vector of chickpea phyllody.
(Courtesy K. P. Akhtar)

**Parasitic Weeds**

**Broomrape**

Chickpea and lentil can be parasitized mainly by two different species
of broomrapes, namely crenate broomrape (*Orobanche crenata* Forsk.) and
Egyptian broomrape (*O. aegyptiaca* Pers. (syn. *Phelipanche aegyptiaca*
(Pers.) Pomel)). Both species have wide host ranges and have been only
reported in anthropogenically disturbed ecosystems, showing a weedy
behavior. In addition, *O. foetida* Poir. has been recently reported
infecting chickpea in Tunisia.

*Orobanche crenata* has been known to threaten legume crops since
antiquity. It is of economic importance in the Mediterranean Basin and
Middle East in lentil and other temperate grain and forage legumes (faba
bean, pea, vetches, grasspea). Chickpea does not suffer important levels
of infection in traditional spring sowings, as it is known that a
delayed sowing reduces the broomrape incidence, but with the continuous
spread of winter sowing, crenate broomrape might become a problem in
chickpea. *O. crenata* can also infect members of Compositae, such as
safflower, and Umbelliferae, such as carrot. It is characterized by
large erect plants, branching only from their underground tubercle. The
spikes may reach up to 1 m high, bearing many flowers of diverse
pigmentation, from yellow, through white to pink and violet (Fig. 1).
The calyx is 13-18 mm, with segments free bidentate. The corolla is
18-28 mm, glandular pubescent, the lips often with lilac veins, lips
divergent, large, not ciliate. The anthers are brown, glabrous or
subglabrous. The filaments insert 2-3(4) mm above base of corolla, and
are hairy at base with glandular hair at apex.

*Orobanche aegyptiaca* parasitizes chickpea and lentil (Fig. 2) but also
many other crops belonging to various families, including Brassicaceae,
Compositae, Cucurbitaceae, Fabaceae, and Solanaceae. It is widely
distributed in eastern parts of the Mediterranean, in the Middle East
and in parts of Asia. It is very similar to *O. ramosa* L. (syn. *Ph.
ramosa* (L.) Pomel) that is more common as a weed in Europe, parts of
Africa and Asia, with some overlap with *O. aegyptiaca* in the northern
parts of the Middle East. However, *O. aegyptiaca* is more aggressive
than *O. ramosa* and adapted to more arid regions. Both species have
branched stems with flowers that may significantly differ in color, from
white to dark blue. Differences may also be found in plant size, which
may be highly branched and reaching 40-50 cm on well-developed hosts,
while in non-irrigated fields they may be much smaller, even 5-10 cm
with only few flowers. A simple feature that allows field distinction is
the hairiness of the stamens at the connective (the sterile tissue
between anthers), which occurs only in *O. aegyptiaca*. The upper leaves
and the corolla in *O. aegyptiaca* are hairy glandular and the lobes of
lower lip of corolla (20-35 mm) are rounded.

*O. foetida* is known as a weed of chickpea only in Tunisia, but the
species is common in native habitats also in other North African
countries and Spain and France. The plant has unbranched stems that bear
red or purple flowers (Fig. 3), which release an unpleasant smell.

**Disease cycle and epidemiology**

Broomrape seeds must undergo conditioning under suitable temperature and
moisture conditions before germination, and they germinate only in
response to a chemical signal from the host root. Optimum temperatures
for conditioning and germination are different among broomrape species,
being about 18C for *O. crenata* and about 23C for *O. aegyptiaca*, with
substantial differences among populations within the species. The
germination process is reversible with desiccation. Even after being
imbibed and conditioned for germination, broomrape seeds can re-enter a
low energy dormant state, if no suitable host is found nearby within a
few days. Whereas primary dormancy coincides with the dry season
directly after maturity, the endogenously induced secondary dormancy
seems to coincide with the subsequent dry seasons. The relatively short
period at which seeds are responsive to stimulants ensures that the
seeds will not germinate too late in the season, when, despite the
presence of a host, the conditions will not allow completion of the life
cycle of the parasite.

*Orobanche* seeds are small (Figs. 4A,B), being less than 1 mm in size,
containing a reduced embryo that is composed solely of a short radicle,
without a plumule and cotyledons. When it germinates only a radicle
emerges out of the tiny seed. The small storage reserves, mainly
composed of lipids, are capable of supporting a few days of autonomous
growth. The emerging radicle (Fig. 4C) grows to a limited extent (few
millimeters). When a root host is reached the radicle tip develops into
an attachment organ called appressorium (Fig. 4D). The intrusive cells
penetrate the host root, ultimately forming a bridge called haustorium
between the vascular systems of host and parasite and the transfer of
nutrients from the host to the parasite is established (Fig. 4E).
Subsequently the parasite develops a tubercle (Figs. 4F,G) that grows
underground on the host root surface for several weeks or months until
it emerge above soil near host plants (Figs. 4H,G) and flowers and sets
seeds (Figs. 4J,A). Unlike other broomrapes that are shelf-pollinating,
both *O. crenata* and *O. aegyptiaca* are believed to be at least
partially outcrossers being pollinated by insects, although they are
able to self-pollinate if not visited by insects. The parasites complete
their life cycle within 7 to 16 weeks and their fruits (capsules) (Fig.
4A) contain seeds already two weeks after pollination, depending on host
phenology. In fact the parasites usually germinate during early stages
of host development, and produce fruits at host maturity. The number of
seeds produced by a healthy *O. crenata* or *O. aegyptiaca* plant can
exceed 200,000 and in exceptionally successful parasites, seed sets may
reach half a million. Large quantities of long-lived seeds assure the
parasite genetic adaptability to changes in host resistance and cultural
practices. The minute seeds may easily be transferred from one field to
another by cultivation, and also by water, wind, animals, and especially
by vehicles and farming machines. Broomrape seeds may remain viable in
soil for decades. Harvesting parasite shoots in forage crops may also
assist in spreading the seeds if used to feed animals, because their
manure may then be contaminated with parasite seeds, which remain viable
after passing through the alimentary system of animals.

### Management

There is no single technology to control *O. crenata* or *O.
aegyptiaca*. So far, the effectiveness of conventional control methods
is limited due to numerous factors in particular the complex nature of
the host-parasite association, the tiny and long-living seeds, and
difficulty in diagnosis until irreversible damage occurs. The intimate
connection between host and parasite also hinders efficient control by
herbicides. The only way to cope with the weedy root parasites is
through an integrated approach, employing a variety of measures in a
concerted manner, starting with containment and sanitation, direct and
indirect measures to prevent the damage caused by the parasites, and
finally eradicating the parasite seedbank in soil. Seedbank demise can
be efficiently achieved by fumigation or solarization, however, this is
not economically feasible in low-value and low input crops like chickpea
and lentil. Some biological control agents have shown promise in
managing broomrapes, but the technology is not ready yet for commercial
application.

Since no resistant lentil varieties to *Orobanche* are available, the
only recommendation to farmers is the integration of several measures:
use broomrape free seeds, delay on sowing date, use of very early
maturing cultivars that might escape infection, and application of
imidazolinone herbicides at low rates.

Several factors hinder chemical control of broomrape: (1) herbicides are
usually effective only as a prophylactic treatment, but in most cases
the actual infestation level of broomrape in the field is usually
unknown; (2) seeds continuously germinate throughout the season; (3) the
parasite is directly connected to the host, therefore, herbicides have
to be selectively against the parasite without causing phytotoxicity on
host plants.; (4) herbicide treatments have to be adapted and applicable
to the diverse broomrape life cycles, to different showing dates and
climatic factors. It has been shown that good broomrape control can be
achieved in faba bean by glyphosate at low rates. However, insufficient
selectivity is found in lentil, although postemergence treatments of
30-40 g a.i./ha can be tolerated by some cultivars. Lentil tolerates
pre-emergence treatments of imazapyr (25 g a.i./ha) and imazethapyr (75
g a.i./ha) and postemergence treatments of imazaquin (7.5 ml a.i./ha).
Phytotoxicity might be higher in the presence of water stress and vary
with the cultivar of lentils.

Crop rotation is of little value due to the persistence of the seeds for
extended periods and the broad host range. There is also promise in a
number of strategies such as suicidal germination by application of
germination stimulants or by the use of trap or catch crops, which have
not proven to be economical. An alternative might be intercropping that
is widely recommended for *Striga* control on maize and sorghum in
Africa, and has recently shown to reduce *O. crenata* infection in
legumes.

Breeding for resistance is the most economic, feasible and environment
friendly method of control. However, resistance against broomrape is
difficult to access, scarce, of complex nature and of low heritability,
making breeding for resistance a difficult task. In spite of these
difficulties, significant success has been achieved in some other crops,
such as sunflower against *O. cumana*, or faba bean and vetch against
*O. crenata*. However, no sources of resistance are available in lentils
until the recent findings of resistant germplasm with resistance based
on a combination of escape and resistance mechanisms. Accessions have
been identified that escape infection due to lower root density; that
induce lower seed germination; that hamper establishment of broomrape
radicles in contact with host roots limiting development of established
tubercles. In addition, necrosis of tubercles was observed in some
accessions. This can be exploited in lentil breeding. Combination of
different resistance mechanisms into a single cultivar should provide a
more durable resistance. This can be facilitated by the adoption of
marker-assisted selection techniques, together with the use of in vitro
screening methods that allow dissecting parasitic weed resistance into
highly heritable components.

In chickpea, resistance is common in germplam and wild species of
*Cicer* and this may be used in breeding programs. The resistance is the
result of the combination of several mechanisms, including low induction
of parasite seed germination and in some accessions either a darkening
at the infection site on the host root that prevents establishment, or a
reduced development of established parasite tubercles, similar to those
observed in lentil.

**Dodder** (*Cuscuta*)

Dodder is a problem in some areas of the Middle East, and is a threat to
chickpea and lentil in certain locations. The most important species is
*Cuscuta campestris*. The stem of the parasite is tough, curling,
leafless and bears only minute scales in place of leaves (Fig. 5). Gray
to reddish brown seeds are produced in abundance and mature within a few
weeks from bloom, Seeds may germinate immediately after they fall to the
ground, or may remain dormant until the following season.
Dodder-infected areas appear as patches in the field and continue to
enlarge during the growing season. In late spring and early summer,
dodder produces a massed cluster of white flowers. Infected host plants
become weakened, decline in vigor and produce poor yields. Several
patches might coalesce to form large areas that can be easily recognized
by the yellowish color of the parasite strands.

An efficient management starts by the use of dodder-free seed and spray
first patches with contact herbicides to prevent spread. Application of
pendimethalin at 1.0 kg/ha as pre-emergence was found safe and effective
against *Cuscuta* in lentil. In chickpea, *C. campestris* is selectively
controlled by pre-emergence application of propyzamide (0.5-0.75 ka
a.i./ha), pronamide (2.5 kg/ha) or pendimethalin (1.0 kg/ha) or by
pre-sowing application of Weedazol (Aminotriazol+ammonium thiocyanate)
at 1250-2500 g a.i/ha. Soil solarization effectively reduces dodder seed
bank in the soil.

References

Arjona-Berral, A., Mesa-García, J., and García-Torres, L. 1988.
Herbicide control of broomrapes in peas and lentils. FAO Plant Prot.
Bull. 36: 175-78.

Fernández-Aparicio, M., Sillero, J. C., and Rubiales, D. 2007.
Intercropping with cereals reduces infection by *Orobanche crenata* in
legumes. Crop Protection 26: 1166-1172.

Joel, D. M., Hershenhorn, Y., Eizenberg, H., Aly, R., Ejeta, G., Rich,
P. J., Ransom, J. K., Sauerborn, J., and Rubiales, D. 2007. Biology and
management of weedy root parasites. Horticultural Reviews 33:267-350.

Linke, K. H., Abd El-Moneim, A. M., and Saxena, M. C. 1993. Variation in
resistance of some forage legumes species to *Orobanche crenata* Forsk.
Field Crops Research*,* 32: 277-285.

Linke, K. H., Singh, K. B., and Saxena, M. C. 1991. Screening technique
for resistance to *Orobanche crenata* Forks. in chickpea. Internat.
Chickpea Newslett. 24: 32-34.

Rubiales, D., Alcántara, C., and Sillero, J. C. 2004. Variation in
resistance to crenate broomrape (*Orobanche crenata*) in species of
*Cicer*. Weed Research 44: 27-32.

Rubiales, D., Alcántara, C., Pérez-de-Luque, A., Gil, J., and Sillero,
J. C. 2003. Infection by crenate broomrape (*Orobanche crenata*) in
chickpea *(Cicer arietinum*) as influenced by sowing date, weather
conditions and genetic resistance. Agronomie 23: 359-362.

Rubiales, D., Pérez-de-Luque, A., Fernández-Aparicio, M., Sillero, J.
C., Román, B., Kharrat, M., Khalil, S., Joel, D. M., and Riches, C.
2006. Screening techniques and sources of resistance against parasitic
weeds in grain legumes. Euphytica 147: 187-199.

Sauerborn, J., Masri, H., Saxena, M. C., and Erskine, W. 1987. A rapid
test to screen lentil under laboratory conditions for susceptibility to
*Orobanche*. Lens Newsletter 14: 15-16.

(Prepared by D. Rubiales, M. Fernández-Aparicio, and J. C. Sillero).

Figures

![](media/image8.png){width="2.999212598425197in"
height="2.25in"}![](media/image9.jpeg){width="1.7133858267716535in"
height="2.2838582677165356in"}

Fig. 1. *Orobanche crenata* on lentil (A) and chickpea (B). (Courtesy D.
Rubiales)

![](media/image10.jpeg){width="2.275in" height="3.5416666666666665in"}

Fig. 2. Branched *Orobanche aegyptiaca* on lentil (Courtesy A. Haddad).

![](media/image11.png){width="2.0in" height="2.7194444444444446in"}

Fig. 3. Unbranched stem with purple flowers of *Orobanche foetida* on
chickpea (Courtesy Mohammed Kharrat).

![](media/image12.png){width="6.38125in" height="9.029861111111112in"}\
Individual photos are available to reset the figure and make changes to
the legends.(W.Chen)

changes to legend. C. remove "with". D. change "and" to "an"

![](media/image13.png){width="2.91259842519685in"
height="2.1854330708661416in"}![](media/image14.png){width="1.7090551181102362in"
height="2.206299212598425in"}

Fig. 5. Leafless, yellowish stems of *Cuscuta campestris* parasitizing
lentil (A) and chickpea (B) (Courtesy of Mónica Fernández-Aparicio).